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Citation McFedries, Amanda Kathryn. 2014. Characterization of Protein-Metabolite and Protein-Substrate Interactions of Disease Genes.Doctoral dissertation, Harvard University.
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iii
Dr. Alan Saghatelian Amanda Kathryn McFedries
Characterization of Protein-Metabolite and Protein-Substrate Interactions of Disease Genes
Abstract
Discovery of protein-metabolite and protein-substrate interactions that can specifically
regulate genes involved in human biology is an important pursuit, as the study of such
interactions can expand our understanding of human physiology and reveal novel therapeutic
targets. The identification and characterization of these interactions can be approached from
different perspectives. Chemists often use bioactive small molecules, such as natural products
or synthetic compounds, as probes to identify therapeutically relevant protein targets.
Biochemists and biologists often begin with a specific protein and seek to identify the
endogenous ligands that bind to it. These interests have led to the development of methodology
that relies heavily on synthetic and analytical chemistry to identify interactions, an approach that
is complemented by in vivo strategies for validating the biological consequences of specific
interactions.
Untargeted metabolomics is a powerful strategy for the identification of novel protein-
small molecule interactions from various tissues that are relevant to target protein function
during normal activity or within the context of a disease state. Here, this platform was used to
identify the first endogenous ligands, prostaglandins A2, B2, D2 and E2, for the orphan nuclear
receptor Nurr1, a gene that is also linked to Parkinson’s Disease. These ligands function as
inverse agonists of Nurr1 transcriptional activity and PGD2 and PGE2 have also been
implicated in the neuroinflammatory pathway that contributes to PD progression.
Further demonstrating the value of these approaches in answering important chemical
and biological questions, the work presented here on targeting the insulin degrading enzyme
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(IDE) in the context of diabetes, illustrates the effectiveness of using small molecule tools to
identifying novel endogenous substrates that play important roles in glucose homeostasis. Here
the first potent and physiologically active IDE inhibitor was to discover that IDE regulates the
abundance and signaling of glucagon and amylin, in addition to that of insulin. Importantly,
under physiologic conditions that augment insulin and amylin levels acute IDE inhibition can
lead to substantially improved glucose tolerance and slower gastric emptying. These findings
transform our understanding of IDE’s roles in glucose regulation, and demonstrate a potential
therapeutic strategy of modulating IDE activity to treat type-2 diabetes.
v
Acknowledgements
I would like to thank Dr. Alan Saghatelian for all the support and guidance he has given
me throughout the years. I am grateful for and appreciate all that I have learned while in his lab
and I am especially thankful for Alan’s ability to gather together such a bright and amazing
group of labmates. Each member of the Saghatelian lab has helped me to succeed, in their own
special way, and has made a positive impact on my life. This intelligent and diverse group of
people made my graduate school experience rich with memory and exceedingly enjoyable.
Thank you all for the love, support and guidance you have given me. I have learnt so much from
each one of you.
This sentiment can easily be extended to all the members of Dr. David Liu’s lab and to
my classmates in the Molecular and Cellular Biology Department. Thank you all for the support,
the fun, and the great scientific discussions. These years would have been pretty boring without
Laila Akhmetova, Kyle McElroy, and Jamie Webster in particular.
I’d especially like to thank those with whom I’ve had the opportunity to collaborate with
scientifically, especially Dr. Erin Adams, Dr. Yihong Wang, Dr. Sam Gellman, Dr. David Liu and
Juan Pablo Maianti.
I would like to thank the faculty and the administration of the MCB department for being
a consistent and dependable guiding force throughout all of my graduate school years. In
particular Mike Lawrence, without him I’m sure the department would fall apart.
I’d like to thank my thesis committee, Dr. David Liu, Dr. Nathanael Gray and Dr. Andres
Leschziner for their guidance and scientific discussions over the years, which have helped me
to grow and succeed as a researcher.
Finally, I would like to thank my loving family for their support and generosity, especially
my husband Tim Hawkins. Without you all I would not be the person that I am today.
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Table of Contents Abstract ....................................................................................................................................................... iii
Acknowledgements .................................................................................................................................... v
Table of Contents ...................................................................................................................................... vi
List of Figures .......................................................................................................................................... viii
List of Tables ............................................................................................................................................... x
List of Abbreviations.................................................................................................................................. xi
Chapter 1 Methods for the Elucidation of Protein-Small Molecule Interactions................................ 1
1.1 Introduction ....................................................................................................................................... 2
1.2 Small-molecule affinity methods.................................................................................................... 2
1.3 Proteomic target identification ....................................................................................................... 6
1.4 Chemoproteomic target identification ......................................................................................... 10
1.5 Biophysical identification of small molecule binders ................................................................ 13
1.6 Affinity-based identification of small molecule binders ............................................................ 15
1.7 Future Directions ........................................................................................................................... 20
1.8 References ..................................................................................................................................... 20
Chapter 2 Metabolomics Strategy Discovers Endogenous Inverse Agonists of the Orphan
Nuclear Receptor Nurr1 .......................................................................................................................... 26
2.1 Introduction ........................................................................................................................... 27
2.2 Identify natural ligands for Nurr1 through an untargeted metabolomics approach ............. 30
2.3 Conclusions .................................................................................................................................... 37
2.4 Methods .......................................................................................................................................... 38
Chapter 3 Anti-Diabetic Activity of Insulin-Degrading Enzyme Inhibitors Mediated by Multiple
Hormones .................................................................................................................................................. 46
3.1 Introduction ..................................................................................................................................... 47
3.2 Potent and selective IDE inhibitors ............................................................................................ 48
3.3 Structural basis of IDE inhibition ................................................................................................. 51
3.4 Inhibition of IDE in vivo ................................................................................................................. 54
3.5 Anti-diabetic activity of IDE inhibition during oral glucose administration ............................. 55
3.6 IDE inhibition during an injected glucose challenge leads to impaired glucose tolerance . 59
3.7 IDE regulates multiple hormones in vivo .................................................................................... 60
3.8 IDE inhibition promotes glucagon signaling and gluconeogenesis ........................................ 62
vii
3.9 IDE inhibition promotes amylin signaling and gastric emptying ............................................. 65
3.10 Implications................................................................................................................................... 66
3.11 Methods ........................................................................................................................................ 68
3.12 References ................................................................................................................................... 83
Appendix 1 Metabolomics Experiments to identify E.Coli derived ligand of MR1 .......................... 90
A1.1 Introduction .................................................................................................................................. 91
A1.2 Results .......................................................................................................................................... 91
A1.3 Methods ........................................................................................................................................ 94
Appendix 2 Evaluation of Potent α/β -Peptide Analogue of GLP-1 with Prolonged Action In Vivo
.................................................................................................................................................................... 95
A2.1 Introduction .................................................................................................................................. 96
A2.2 Results .......................................................................................................................................... 96
A2.3 Discussion .................................................................................................................................... 99
A2.4 Method .......................................................................................................................................... 99
A2.5 References ................................................................................................................................. 100
Appendix Chapter 3 Supplementary Data .......................................................................................... 104
viii
List of Figures
Figure 1.1 Affinity capture coupled to SILAC for small molecule target identification ……………4
Figure 1.2 Drug Affinity Responsive Target Stability (DARTS) ……………………………………..7
Figure 1.3 Stability of Proteins From Rates of Oxidation (SPROX) ………………………………..9
Figure 1.4 Identifying protein targets in cell culture ………………………………………………..12
Figure 1.5 Thermostability Shift Assay ……………………………………………………………….15
Figure 1.6. Affinity methods for elucidating PMIs …………………………………………………...18
Figure 2.1 Ligands for the NR4A receptors ……………………………………………………........30
Figure 2.2 A liquid chromatography-mass spectrometry (LC-MS)-based metabolomics approach
for characterizing endogenous nuclear receptor (NR) ligands …………………………………….32
Figure 2.3 Circular Dichroism of Nurr1-LBD and candidate ligands ………………………………33
Figure 2.4 Intrinsic tryptophan fluorescence screen for lipid binding by Nurr1-LBD …………….36
Figure 2.5 Saturation binding curves using intrinsic tryptophan fluorescence …………………..37
Figure 3.1 Discovery of potent and highly selective macrocyclic IDE inhibitors from the in vitro
selection of a DNA-templated macrocycle library……………………………………………………49
Figure 3.2 Structural basis of IDE inhibition by macrocycle 6b ……………………………………52
Figure 3.3 Physiological consequences of acute IDE inhibition by 6bK on glucose tolerance in
lean and DIO mice .……………………………………………………………………………………..58
Figure 3.4 Acute IDE inhibition affects the abundance of multiple hormone substrates and their
corresponding effects on blood glucose levels ………….…………………………………………..61
Figure 3.5 Acute IDE inhibition modulates the endogenous signaling activity of glucagon, amylin
and insulin …………………………………………………………………………….…………………64
Figure 3.6 Model for the expanded roles of IDE in glucose homeostasis and gastric emptying
based on the results of this study …………………………………………………...………………..67
Figure A1.1 MAIT Recognition of a Stimulatory Bacterial Antigen Bound to MR1 ………………93
ix
Figure A2.1 α/β-peptide 6 demonstrates long lasting improvement of in vivo
glucose tolerance ……………………………………………………………………………………115
Figure A3.1 Inhibitor Selection Scheme ……………………………………………………………122
Figure A3.2 Inhibition of human and mouse IDE activity demonstrated using distinct assays..123
Figure A3.3 Data collection and refinement statistics (molecular replacement), docking …….124
simulation for 6b, and competition test between insulin and fluorescein-labeled macrocycle 31
for binding CF-IDE …………………………………………………………………………………....125
Figure A3.4 Small molecule-enzyme mutant complementation study to confirm the macrocycle
binding site and placement of the benzophenone and cyclohexyl building-block groups …….126
Figure A3.5 Pharmacokinetic parameters of 6bK …………………………………………………127
Figure A3.6 Dose tolerance, augmented insulin hypoglycemic action by 6bK in mice, and
unaffected amyloid peptide levels in the mouse brain ……………………………………………128
Figure A3.7 Dependence of insulin and glucagon secretion on the route of glucose
administration (oral or i.p.) due to the both the ‘incretin effect’ as well as the hyperinsulinemic
phenotype of DIO versus lean mice ………………………………………………………………129
Figure A3.8 Low-potency diastereomers of 6bK used to determine effective dose range of 2
mg/mouse and confirm on-target IDE inhibition effects during IPGTTs in lean and DIO mice .130
Figure A3.9 Relative area under the curve calculations and 6bK dose response for the glucose
tolerance tests shown in Fig. 3.3 ………………………………………………………………….131
Figure A3.10 Oral glucose tolerance of mice lacking IDE compared to WT lean mice, and lack of
effect of 6bK treatment in IDE–/– knockout mice …………………………………………………134
x
List of Tables Table 2.1 Negative mode ions that are enriched by Nurr1-LBD …………………………………..33
Table A3.1 Literature survey of putative IDE substrates identified using in vitro assays ……..137
Table A3.2 HPLC and high-resolution mass spectrometry analysis of IDE inhibitor analogs ..138
Table A3.3 Site-directed mutagenesis primers ……………………………………………………140
Table A3.5 Site-directed IDE mutants used in the small molecule-enzyme mutant
complementation studies …………………………………………………………………………….141
xi
List of Abbreviations
ACE angiotensin converting-enzyme
cdiGMP bis-(3’-5’)-cyclic dimeric guanosine monophosphate
CRABP2 cytosolic retinoic acid binding protein 2
CsA cyclosporine A
CsnB cytosporone B
CuACC copper-catalyzed cycloaddition of azides and alkynes
DART drug affinity responsive target stability
DBD DNA binding domain
DGC diguanylate cyclase
DIO diet-induced obese
DPP4 dipeptidyl peptidase 4
DNA deoxyribonucleic acid
DRaCALA differential radial capillary action of ligand assay
DSF differential scanning fluorimetry
DSLS differential static light scattering
ERα estrogen receptor alpha
ESI-TOF electrospray ionization time of flight mass spectrometry
FABP2 fatty acid binding protein 2
FPLC fast protein liquid chromatography
G6Pase glucose-6-phosphatease
GCGR G-protein coupled glucagon receptor
GLP-1 glucagon-like peptide 1
GLP-1 glucagon-like peptide 1
GPCR G-protein coupled receptors
GST glutathione s-transferase
xii
GTT glucose tolerance test
His6 polyhistidine
His6-Nurr1-LBD His6-tagged-Nurr1LBD
IDE insulin-degrading enzyme
IPGTTs injected glucose tolerance tests
IPTG isopropyl-B-D-1-thiogalactopyranoside
ITT insulin tolerance tests
Kd dissociation constant of the protein-ligand complex
LC-MS liquid chromatography–mass spectrometry
MetE S-methyltransferase
MMP1 matrix metalloprotease 1
MRM multiple reaction monitoring
MudPIT multidimensional protein identification technology
MW molecular weight
MWCO molecular weight cutoff
m/z mass-to-charge ratio
nat-20(S)-yne 20(S)-hydroxycholesterol
NEP neprilysin
NLN neurolysin
NR nuclear receptor
NR4A nucleasr receptor subfamily 4A
OGTT oral glucose tolerance tests
OD600 optical density at 600 nm
PBS phosphate buffered saline
PCR polymerase chain reaction
PEPCK phosphoenolpyruvate carboxykinase
xiii
PMI protein-metabolite interactions
PSMI protein-small molecule interactions
PTT pyruvate tolerance test
ROS reactive oxygen species
SEC size exclusion chromatography
Shh sonic hedgehog
SILAC small molecule-affinity chromatography with stable isotope labeling of
amino acids in cell culture
Smo smoothened
SMTA s-methyl thioacetimidate
SPROX stability of proteins from rates of oxidation
StarD3 stAR-related lipid transfer domain protein 3
TBS tris-buffered saline
T2D type-2 diabetes
THOP thimet oligopeptidase
Tm melting temperature
UFA unsaturated fatty acid
WT wildtype
1
Chapter 1
Methods for the Elucidation of Protein-Small Molecule Interactions
This chapter was adapted from:
McFedries, A, Schwaid, A, Saghatelian, A. Methods for the Elucidation of Protein-Small
Molecule Interactions. Chem Biol. 20, 667-73 (2013)
2
1.1 Introduction
A number of different types of molecular interactions enable life. These include the
interactions between proteins, proteins and nucleic acids, and proteins and small molecules.
Elucidating these interactions and understanding how they control biology is a major scientific
goal. A number of approaches have been developed in recent years to identify protein-protein
interactions [1-6] and protein-nucleic acid interactions [7-9]. Ribosome profiling, for example,
elucidates interactions between the ribosome and RNA in cells to reveal novel sites of protein
translation. While many methods exist for the characterization of biopolymer interactions, far
fewer approaches exist to elucidate interactions between proteins and small molecules. In
recent years, however, more of these methods are beginning to emerge.
The importance of protein-small molecule interactions (PSMIs) in drug discovery and
protein-metabolite interactions (PMIs) in biology has driven the development of new methods
that rely heavily on the integration of both synthetic chemistry and analytical chemistry. Here,
we divide these methods into two categories: small molecule-to-protein and protein-to-small
molecule strategies. This division separates problems that aim to identify the protein targets of a
bioactive small molecule from problems focused on identifying the small molecule-binding
partner of a suspected metabolite-binding protein.
1.2 Small-molecule affinity methods
One of the successes in using small molecules as affinity reagents is the identification of
FKBP by the natural product FK506 [10]. This seminal work led to the discovery of new proteins
and pathways that explained the mechanism of action of a potent class of immunosuppressant
drugs [11]. In doing so, this work informed us about vital, but previously unknown, cellular
pathways involved in the regulation of the cellular immune response. More generally, these
studies highlighted the tremendous value of using bioactive small molecules to study biology.
Other important examples, including the discovery of the histone deacetylase family with
3
trapoxin [12], reinforced the impact of chemistry in important biological discoveries, leading to
the development of the field of chemical biology [13]. All of this is predicated on being able to
use complex bioactive small molecules as affinity reagents, which often requires complex
chemical syntheses and emphasizes the importance of organic chemistry in this problem.
The increased use of small molecule screening approaches in biology has led to the
identification of many bioactive molecules, leading to an increased demand for methods that
can elucidate PSMIs. Affinity-based methods are still the most common approach used and
leading methods have learned to integrate these approaches with modern proteomics to
accelerate targeted discovery. Ong and colleagues, for example, have combined small
molecule-affinity chromatography with stable isotope labeling of amino acids in cell culture
(SILAC) [14], a quantitative mass spectrometry (MS)-based proteomics strategy (using an ion
trap MS), to identify PSMIs on a proteome-wide scale [14, 15] (Figure 1.1). To demonstrate the
generality of this approach seven different compounds, including kinase inhibitors and
immunophilin ligands, were studied in this first example. Derivatives of each of these
compounds were prepared and linked to solid support by a carbamate linkage, affording small
molecule derivatized beads.
4
Figure 1.1 Affinity capture coupled to SILAC for small molecule target identification. Cells
are grown in ‘heavy’ or ‘light’ media and subsequently lysed. These ‘heavy’ and ‘light’ cell
lysates are separately incubated with beads that are modified with a small molecule of interest.
Excess small molecule is added to the ‘light’ cell lysate and this soluble small molecule prevents
any specific small molecule-protein interactions with the beads. After removal of the lysate
bound proteins are eluted from the beads and the lysates are then combined for subsequent
analysis using quantitative proteomics. The samples can be distinguished by mass
spectrometry since proteins from each sample have different molecular weights, and therefore
specific PMSIs can be identified by the higher concentrations of these ‘heavy’ proteins versus
‘light’ proteins.
In SILAC, cells are then grown in regular media (light) or specialized media (heavy) that
replaces certain amino acids with stable isotope labeled derivatives (e.g. 13C6-arginine and
13C6,15N2-lysine). The result is that the proteins in the ‘heavy’ cells have proteins that weigh
5
more than the exact same proteins in ‘light’ cells, and these proteins can be distinguished and
quantified by mass spectrometry. SILAC is used to identify PSMIs by passing ‘light’ lysate over
beads coated with the bioactive small molecule. Any proteins with affinity for the small molecule
are retained. As a control, a soluble variant of the small molecule is added to the ‘heavy’ lysate
before it is incubated with the small molecule-modified beads. This soluble compound has the
effect of binding the target proteins and preventing their binding to the small molecules on the
surface of the bead. The post-bead lysate samples are then combined and analyzed by mass
spectrometry. The ratio of light-to-heavy can identify those proteins that are specifically enriched
by the small molecule on the bead, and therefore identify any target proteins of the small
molecule.
The results from these initial experiments were excellent. All the compounds used
identified known PSMIs, and several revealed some novel interactions. Moreover, by using
compounds with different affinities for their targets, this work demonstrated that this method can
successfully identify PSMIs with affinities from the low nanomolar (26 nM) to micromolar (44
μM) range. This strategy has been applied to the identification of the primary targets of
piperlongumine [16], a compound that was shown to selectively kill cancer cells in vitro and in
vivo by targeting the stress response to reactive oxygen species (ROS) [17]. Overall, these
types of affinity approaches have come to dominate the methods that are used to identify
PMSIs. Examples include the identification of the nucleophosmin as a target of natural product
avrainvillamide [18], the finding that cephalostatin A binds to specifically to members of the
oxysterol binding-proteins, in the process revealing these proteins to be important in cancer cell
proliferation[19].
Importantly, affinity methods are not limited to synthetic compounds or natural products,
but can also be used with endogenous metabolites. Specifically, Nachtergaele and colleagues
demonstrated a direct binding interaction between 20(S)-hydroxycholesterol and the
oncoprotein smoothened (Smo), a key protein in the sonic hedgehog (Shh) pathway, using a
6
derivative of 20(S)-hydroxycholesterol (nat-20(S)-yne) that was immobilized onto a solid support
using Sharpless’ click chemistry [20]. This example highlights the generality of affinity-based
approaches in identifying PSMIs. The only limitation appears to be the ability to access
derivatives for immobilization by chemical synthesis and compounds that have or retain high
affinity for their protein target. As scientists continue to gain interest in understanding the
mechanism underlying bioactive small molecules, affinity-based methods will continue to be
applied to many more target molecules.
1.3 Proteomic target identification
In cases where small molecules are difficult to modify, or the synthetic skill necessary to
make such modifications are difficult to access, a new group of powerful proteomics methods to
discover novel PSMIs can be used. These strategies rely on detecting differences in the stability
between unbound and small-molecule bound proteins to identify the target(s) of a small
molecule. Drug affinity responsive target stability (DARTS) is one such method [21].
DARTS relies on the fact that proteins are more stable when bound to a metabolite,
which makes them less susceptible to proteolysis. Lysates are compared in the presence and
absence of a small molecule. Proteins that bind to the small molecule are protected from
proteolysis relative to the control sample, as indicated by mass spectrometry (Figure 1.2). Proof-
of-concept experiments revealed that mammalian target of rapamycin (mTOR), for example, is
less susceptible to proteolysis in the presence of E4, an mTOR kinase inhibitor. Moreover,
DARTS is generally applicable and was used with other enzyme-inhibitor pairs, such as the
COX2-celecoxib pair.
7
Figure 1.2 Drug Affinity Responsive Target Stability (DARTS). Aliquots of a protein lysate
are mixed with either a small molecule (+ ligand) or solvent control (-ligand) to identify PSMIs.
These samples are then subjected to limited proteolysis and compared by gel electrophoresis
and quantitative mass spectrometry. Protein targets are identified as those proteins that display
increased protease resistance in the presence of the small molecule.
Next, DARTS was used to characterize PSMIs for resveratrol, an anti-aging compound
thought to act primarily through interactions with the sirtuin protein Sir1. Using a yeast and
human lysates the authors discovered that eukaryotic initiation factor A (eIF4A) is a target of
resveratrol, which demonstrates that DARTS is able to discover novel PSMIs. Importantly, the
authors confirmed that at least some of the biology controlled by resveratrol is eIF4A dependent
8
because worms lacking eIF4A no longer show any anti-aging in the presence of resveratrol.
Together these experiments demonstrate the value and utility of DARTS for discovering PSMIs.
Most recently, a proteomics method called Stability of Proteins from Rates of Oxidation
(SPROX) was developed to identify PSMIs in complex cell lysates [22-25]. Rather than relying
on non-specific proteolysis, which can make downstream mass spectrometry experiments
difficult to interpret, SPROX relies on the irreversible oxidation of methionine residues by
hydrogen peroxide to report on the thermodynamic stability of a protein’s structure during
chemical denaturation (Figure 1.3). Proof-of-concept SPROX experiments performed using
yeast lysates validated this approach by identifying known binders of the immunosuppressant
drug cyclosporine A (CsA) [23]. SPROX has also been used with resveratrol, identifying the
known target, cytosolic aldehyde dehydrogenase, along with several novel interactions [25].
SPROX requires that target proteins contain methionine residues, and multidimensional protein
identification technology (MudPIT) [26, 27] analysis of SPROX experiments using yeast lysates
demonstrated that 33% of the detectable proteins contain a methionine.
9
Figure 1.3 Stability of Proteins From Rates of Oxidation (SPROX). SPROX identifies the
targets of a small molecule from a complex protein mixture by measuring the ligand-induced
changes in the rate of methionine amino acid side chain oxidation by hydrogen peroxide.
Aliquots of the cell lysate are incubated with either a small molecule or a solvent control and
then incubated with increasing concentrations of guanidine hydrochloride.
Ligand induced difference in target protein unfolding will impact the rate of selective methionine
oxidation by hydrogen peroxide. Quantitative proteomic is used to compare levels of reduced
versus oxidized methionine-containing peptides in each sample set (small molecule versus
control) to determine the rate of target protein oxidation as a function
of guanidine hydrochloride concentration. A shift of the transition midpoint for a protein between
+ligand and –ligand samples indicates that the protein is a target for the small molecule in
lysate.
A SPROX-like method that uses s-methyl thioacetimidate (SMTA) labeling to detect
amidination differences of proteins and protein-ligand complexes during chemical denaturation
has also been explored [28]. This method requires target proteins to contain lysine residues or
have a buried N-terminus in the native state. This method is particularly useful when a ligand of
interest is not stable in hydrogen peroxide and therefore cannot be investigated by SPROX.
10
SMTA labeling and SPROX complement each other, covering a wider range of the proteome
[28]. Studying the thermodynamic stability of proteins under denaturing conditions in the
presence and absence of ligand is an effective target protein identification strategy. However,
the two described approaches require relatively large concentrations of ligand, in the uM to mM
range, although they provide the flexibility to use a variety of downstream quantitative proteomic
techniques.
1.4 Chemoproteomic target identification
Unfortunately, not all proteins are as active in lysates as they are within the context of a
cell, and therefore some relevant PSMIs or PMIs may be missed when using lysates. Screening
a spiroepoxide library for antiproliferative compounds, for example, revealed that the most
relevant biological target of the active spiroepoxide is only targeted in a living cell, but was
inactive once the cell was lysed [29]. Many molecular mechanisms can account for the
difference between intact cells and lysates but the ultimate point is that it is difficult to exactly
replicate cellular conditions in any type biochemical experiment. Since it is impossible to predict
what PSMIs are sensitive to cellular conditions new chemoproteomic approaches have been
developed to enable target identification within live cells.
These methods rely on the use of small molecules that can covalently label their protein
targets so that intracellular labeling events can be detected after cell lysis. Manabe and
colleagues demonstrated the value of this approach with a modified natural product derivative in
an effort to identify its protein target [30]. Potassium isolespedezate, a metabolite known to
induce nyctinastic leaf opening in the motor cells of plants belonging to the Cassia genus, was
derivatized with an iodoacetamide for covalent crosslinking to its target and an azide to enable
enrichment and identification of the isolespedezate target by conjugation to a flag peptide using
click chemistry. This approach led to the identification of 5-methyltetrahydropteroyltriglutamate-
homocysteine S-methyltransferase (MetE) as the isolespedezate target protein. This method,
11
while powerful, is mostly limited by the ability to synthesize natural product derivatives that can
covalently label their target while maintaining the potency of the compound.
Most recently, a chemoproteomic strategy approach was developed for the identification
of PMIs for the endogenous metabolite cholesterol. Cholesterol is a central metabolite with roles
in membrane structure, metabolism, signaling and disease. While many important functions of
this molecule are known, the full spectrum of proteins that interact with cholesterol is far from
complete. Hulce and coworkers synthesized a series of cholesterol derivatives and controls
containing a photocrosslinking diazirine group [31] (Figure 1.4). In practice, cells are irradiated
by light after exposure to these sterol probes resulting in the covalent modification of any protein
they bind. Addition of exogenous cholesterol blocks the overall labeling of these probes to
validate that binding of these probes is occurring at cholesterol-specific binding sites.
Subsequent to probe labeling, the probe is conjugated to biotin by copper-catalyzed
cycloaddition of azides and alkynes (CuACC) [32] chemistry allowing for affinity enrichment of
labeled proteins.
12
Figure 1.4 Identifying protein targets in cell culture. Cells grown in ‘heavy’ and ‘light’ media
are treated with a cholesterol probe compound that has been modified to contain a diazirine
moiety. In addition, excess cholesterol is also added to the ‘light’ sample and this will act to
compete any specific cholesterol probe–protein interactions. The cholesterol probe is
photocrosslinked to any bound protein targets in cells, and the cells are subsequently lysed. Any
cholesterol probe–protein conjugates in this lysate are then modified with biotin using ‘click’
chemistry and labeled proteins are separated from cell lysate by affinity chromatography. The
‘heavy’ and ‘light’ fractions are then mixed and examined by quantitative proteomics. Proteins
that specifically bind cholesterol will have a higher ratio of ‘heavy’ to ‘light’ in the mass spectrum.
13
Integrating these sterol probes with SILAC [14] enables the identification of sterol probe-
target proteins. In these experiments, the probe is added to both ‘heavy’ and ‘light’ cells, but the
‘light’ cells also contain a competitor (cholesterol) to block binding. Subsequent analysis of the
‘heavy’ and ‘light’ samples identifies cholesterol-binding proteins as those proteins enriched in
the heavy sample versus the control sample. The identification of several known cholesterol-
binding proteins such as Scap, caveolin and HMG-CoA reductase validated the methodology.
Subsequent analysis of the entire data set using various bioinformatics tools revealed that
almost every major class of protein has members that bind cholesterol, including GPCRs, ion
channels and enzymes. More broadly, the analysis also revealed an enrichment of proteins
involved in neurological disorders, cardiovascular and metabolic disease, demonstrating the
potential therapeutic insights that may eventually be provided by this data.
Together these examples demonstrate the utility of chemoproteomic approaches to
identify PSMIs and PMIs, and highlight the power of these approaches to rapidly increase our
understanding about the role of specific small molecules in biology.
1.5 Biophysical identification of small molecule binders
In many cases, the problem of identifying a PMI begins with interest in a particular
protein. This protein may be a potential drug target or it may be suspected to require small
molecule binding to regulate its activity. There are numerous cell-based assays for GPCRs [33-
35] and nuclear receptors [36], for example. In general, these methods are highly effective.
Such assays have already been reviewed extensively in the literature [33-36]. Instead, we’ve
decided to focus on cell-free approaches that rely heavily on biochemical, biophysical and
profiling methods to reveal PMIs for endogenous metabolites.
Biophysical screening methods provide an effective means for PMI discovery from
endogenous metabolites. Differential scanning techniques were originally developed to optimize
recombinant protein stability (i.e. melting temperature (Tm)) for purification and crystallography
14
[37]. Differential static light scattering (DSLS) and/or differential scanning fluorimetry (DSF) are
the two most commonly used methods. DSLS measured denaturation by tracking temperature
induced increases in the intensity of scattered light, while DSF measured increases in the
fluorescence from the environmentally sensitive dye SYPRO Orange. Shifts in melting
temperatures of > 2 °C were found to confidently represent binding events and conditions that
enhanced protein stability, and thermal shifts > 4 °C increased the likelihood of positive results
in crystallographic screens.
These methods have recently been extended to identify PMIs by measuring the effect of
small molecules on the melting temperature (Tm) of proteins. The binding between a small
molecule and protein stabilizes the protein structure (i.e. raises the Tm) (Figure 1.5). Recently,
DeSantis and coworkers used DSF to identify natural estrogen receptor alpha (ERα) ligands
from a library of molecules (not from a complex mixture) [38] . DSF successfully identified
known natural ERα agonists, β-estradiol and estrone, demonstrating the utility of this assay in
characterizing natural PMIs. The authors suggest that these assays will be useful in the
identification of unknown nuclear receptor ligands in the future.
15
Figure 1.5 Thermostability Shift Assay. PSMI and PMIs can be identified in a high-
throughput fashion by monitoring shifts in the melting temperature (Tm) of a protein-ligand
complex versus a protein-solvent control. The environmentally sensitive dye SYPRO Orange
emits when bound to hydrophobic amino acid residues and is used to monitor protein unfolding
via differential scanning fluorimetry (DSF).
1.6 Affinity-based identification of small molecule binders
Alternatively, affinity based experiments using immobilized proteins are another option
for the characterization of PMIs. In general, these assays provide the advantage that they can
be performed with unmodified metabolite resulting in a reduced likelihood of false negatives.
This approach relies on the fact that proteins can be immobilized without altering the secondary
structure of the protein or interfering with ligand binding. The first examples of affinity methods
relied on using radioisotopes to identify PMIs by measuring radioactivity of a protein after
incubation and washing with a radiolabeled ligand [39, 40].
16
Most recently, this approach has been optimized in the form of a DRaCALA assay
(Differential radial capillary action of ligand assay), which allows for the rapid high throughput
identification of PMIs using radiolabeled metabolites [41]. DRaCALA utilizes the affinity of
proteins for nitrocellulose membranes to sequester radiolabeled metabolites bound to protein.
A solution containing the protein of interest and radiolabeled ligand is spotted on nitrocellulose.
Unbound ligand will diffuse with the solvent throughout the membrane, whereas protein and
ligand bound to protein will be immobilized at the point it was spotted. One advantage of
DRaCALA is that it can avoid time-consuming protein purification by using whole cell lysate to
identify PMIs as long as control cell lysate that does not express the metabolite-binding protein
is available.
The one disadvantage of this method is that it requires foreknowledge as to what
candidate metabolites should be tested, and in that each metabolite must be tested individually.
Nevertheless, for certain cases DRaCALA provides a high-throughput means to identify ligand-
binding proteins. The identification of prokaryotes that have proteins capable of binding bis-(3’-
5’)-cyclic dimeric guanosine monophosphate (cdiGMP), a metabolite important in biofilm
formation, was accomplished by simply using lysates from 191 strains of P. aeruginosa and 82
other bacterial strains. The ‘hits’ in this assay corresponded to those bacteria that have
diguanylate cyclase (DGC), as expected. This approach precludes the identification of
unexpected PMIs or PMIs with novel metabolites. Still, DRaCALA remains a powerful approach
for uncovering protein metabolite interactions.
The use of global mass spectrometry approaches allows for the scrutiny of a larger pool
of metabolites, including novel metabolites, and can result in the unbiased identification of
protein metabolite binding. Specifically, the use of global metabolite profiling enabled the
development of a novel, unbiased, strategy for the identification of endogenous PMIs [42]
(Figure 1.6). In this approach, recombinant proteins fused to an affinity tag—either GST or
hexahistidine—are immobilized on a solid support. Incubation of these proteins with a
17
metabolite mixture, typically an extract containing the entire lipidome from a cell or tissue of
interest results in the formation of a protein-metabolite complex on the bead. Following this
incubation, the protein is washed, subsequently eluted from the solid support, and the eluent is
then analyzed using a liquid chromatography–mass spectrometry (LC–MS) metabolite profiling
platform (using an ESI-TOF for the MS). Quantitative comparison of the metabolite profiles
between samples with and without protein reveals any metabolites that are enriched by the
protein.
18
Figure 1.6. Affinity methods for elucidating PMIs. A) Protein (blue) is immobilized on a solid
support (grey) and incubated with lipids from tissue lysate. The immobilized protein is then
washed and the protein is eluted from the beads. The eluate is then analyzed by LC–MS and
compared to eluate from a control sample (solid support with no protein) by in order to identify
specific PMIs. B) A yeast strain bearing either the protein of interest fused to an IgG epitope tag,
or the IgG epitope tag only, was lysed and immunoprecipitated using antibody labeled beads.
Lipids were then extracted from the beads and examined by LC–MS. Comparison between the
protein and control sample can be used to identify any specific PMIs.
This approach was developed using three different lipid-binding proteins with known
ligands: cytosolic retinoic acid binding protein 2 (CRABP2), fatty acid binding protein 2 (FABP2)
and StarD3. The strategy successfully identified specific PMIs for all three of these proteins, and
19
in doing so created a reliable method to pulldown protein metabolite interactions [42]. It does
not require any explicit knowledge about the identity of the metabolite and can be conducted
rapidly against a large pool of metabolites. Moreover, it was not susceptible to the enrichment
of nonspecific metabolites. Although the examples presented here centered on lipids, there is
no reason this approach could not be used for polar metabolites as well. This strategy has been
successfully applied to other PMIs, including the discovery that arachidonic acid and
docosahexanoic acid, polyunsaturated fatty acids, bind to the orphan nuclear receptor Nur77
[43].
Li and colleagues developed an exciting strategy to identify PMIs within yeast [44]
(Figure 1.6). Specifically, they focused on interaction with yeast protein kinases as well as
proteins that comprise ergosterol pathway. The proteins in this group were epitope tagged to
enable their immunoprecipitation of from cellular lysates. These immunoprecipitated samples
were analyzed by metabolomics to identify any endogenous metabolites bound to the proteins.
As a control, each sample was also checked by SDS-PAGE to ensure pulldown of the target
protein was successful.
Comparison of the metabolite profiles from these various samples revealed a number of
new interactions. Many of the enzymes within the ergosterol pathway bound to sterol
intermediates, which suggest that these molecules exert regulation on the pathway.
Interestingly, it was also discovered that some of the proteins within the ergosterol pathway bind
to pentaporphoryin, which was a complete surprise but helps explain a previous observation
linking pentaporphoryin and ergosterol regulation. Furthermore, their analysis led to the
discovery that a number of yeast protein kinases are regulated by ergosterol to highlight the
generality of this method towards numerous protein classes. In aggregate, this data highlights
the potential for unbiased PMI identification to greatly increase our current understanding of
endogenous small molecule biology.
20
1.7 Future Directions
A successful library of approaches to determine PSMIs and PMIs has been developed,
and is ready to be applied to identify unknown PMIs of interest. These approaches enable the
discovery of novel interactions and are also designed to maximize the likelihood that the
interactions are occurring in cells and tissues. The continued application of these methods will
enrich our understanding of small molecule biology and also stimulate the development of
improved methods for discovering these interactions. As demonstrated by the above examples
this research area sits squarely at the interface of chemistry and biology and will greatly benefit
from collaboration between future generations of chemists, biochemists and biologists.
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26
Chapter 2 Metabolomics Strategy Discovers Endogenous Inverse Agonists of the
Orphan Nuclear Receptor Nurr1
27
2.1 Introduction
Nuclear receptors are a family of ligand-dependent transcription factors that respond to
the environment of a cell by binding to a diverse battery of signaling molecules, such as
oxysterols (LXR), vitamin D (VDR), estrogen (ER) and cortisol (GR)1-3. These receptors directly
affect the expression of their target genes and play a central role in regulating genetic programs
that control physiology related with numerous processes, including development and
metabolism 2. In addition to a role in normal physiology, nuclear receptor dysfunction is
associated with diseases such as diabetes and cancer 1, 4. As powerful regulators of physiology
nuclear receptors are also targets of approved drugs, such as Advair (targeting GR for asthma
and COPD) and Avandia (i.e. Rosiglitazone; targeting PPARγ for type II diabetes)5 .
Nuclear receptors have a well conserved domain architecture composed of a highly
variable N-terminal ligand-independent activation function (AF-1), a central DNA binding domain
(DBD), a flexible hinge region and a C-terminal ligand-binding domain (LBD) that contains a
ligand-dependent activation function (AF-2) 1, 6.The DBD contains two well conserved zinc
fingers motifs that mediate receptor binding to specific DNA sequences, called hormone
response elements (HRE), in the promoter region of target genes. The LBD is responsible for
the recognition of the small molecule ligand, receptor dimerization, and the recruitment of co-
regulator proteins to initiate transcription 2. Members of the nuclear receptor superfamily share
structural homology in their ligand binding domain (LBD), which is composed of 12 α-helices
and 2-3 -strands that are arranged as a three layered, antiparallel sandwich 1, 2.
At the molecular level the canonical nuclear receptor uses a conformational change
upon binding of a small molecule ligand to control gene transcription. The mechanism of nuclear
receptor activation can be described as a switch between associations with co-repressor and
co-activator proteins driven by ligand-dependent positioning of the C-terminal alpha helix of the
LDB (helix 12) 6. In the absence of ligand, helix 12 occupies the co-activator binding surface and
28
facilitates co-repressor association with the receptor. Binding of an agonist induces a critical
conformational change in the positioning of helix 12 that leads to the exchange of co-repressor
(SMRT/NCOR and HDAC complexes) for co-activator proteins (HAT and chromatin remodeling
complexes) 6-9 at a hydrophobic interface composed of residues from H12, H3 and H4 1, 10.
Recently, the Saghatelian lab developed a metabolomics approach for elucidating
protein-metabolite interactions and applied this approach to identify candidate endogenous
ligands for the orphan nuclear receptor Nur77 (NR4A1). The NR4A subfamily contains two other
members, Nurr1 (NR4A2) and Nor1 (NR4A3), also considered to be orphans or known
members of the nuclear receptor family that lack any currently accepted ligand 11, 12. We
became interested in this class of nuclear receptors because they are widely expressed in
energy demanding tissues (liver, brain, skeletal muscle and adipose), where they regulate
essential pathways involved in metabolism and development such as gluconeogenesis (Nur77)
11, 13, 14, the development of dopaminergic neurons (Nurr1)15, 16, and lipid, carbohydrate and
energy metabolism (Nor1) 12.
The NR4A subfamily is characterized by atypical LBDs that lack both a canonical ligand
binding pocket and a classical co-regulator interface 10, 17. Previously, Nur77 and Nurr1 were
reported to be constitutively active nuclear receptors that did not have or need a ligand to
function. This conclusion was supported by the apo-LBD crystal structures of Nurr1 (PDB:
1OVL) 10 and Nur77 (PDB: 1YJE, 2QW4) 17 that indicated that the ligand binding domain of the
receptors are filled with large, hydrophobic residues and, therefore, do not require a ligand.
These crystal structures also showed that polar residues that did not associate with co-
regulators populated the classical, hydrophobic, co-regulator interface. However, a novel co-
regulator-binding cleft has been identified, composed of residues from helices 11 and 12. Co-
repressor proteins are capable of interacting with this surface, but to date no co-activator
proteins have been found to bind to the NR4A LBD 18, 19. From this data it appears that the
29
N4RA family is unique in that it does not require a ligand to operate and does not use the
canonical NR co-activators to modulate activity.
However, other data, at least in terms of ligand binding (Figure 1), suggest another story.
First, prostaglandin A2 was identified as a NOR1 agonist through screening 20. This indicates
that there exist endogenous lipids that are able to bind and regulate the activity of members of
the NR4A family. In addition, two small-molecule agonists of Nur77 have been reported,
cytosporone B 21 and 1,1-bis(3-indolyl)-1-(p-methoxyphenyl)methane (BIM) 22, which indicate
that Nur77 transcriptional activity can be regulated by the binding of a small molecule.
Regarding Nurr1, its activity can be activated by both benzimidadole (BEN) 23, 24 and
isoxazolopyridinone (IXP) derivatives 24, but it is unclear if these compounds interact directly
with the receptor. These finding prompted the search for a natural ligand for X using
metabolomics. The application of this strategy revealed that Nur77 binds polyunsaturated fatty
acids (PUFAs; arachidonic and docosahexanoic acids)25. Here, I apply this metabolomics
approach to identify candidate ligands for the NR4A family member Nurr1 and characterize the
impact of lipid binding on the receptor’s transcriptional activity to identify bona fide endogenous
ligands.
30
Figure 2.1 Ligands for the NR4A receptors include the Nor1 agonist prostaglandin A2, the two
Nur77 agonists BIM and Cytosporone B (boxed functional groups have properties reminiscent of
endogenous lipids), and the Nurr1 activating derivatives of benzimidole and
isoxazolopyridinone. Arachidonic acid has recently been identified inverse agonist of Nur77.
2.2 Identify natural ligands for Nurr1 through an untargeted metabolomics approach
To determine candidate ligands for the human Nurr1 receptor an untargeted
metabolomics approach to identify protein-metabolite interactions (Figure 2) 26-28 will be used.
Lipids for this experiments were prepared from mouse brain tissue because Nurr1 activity is
essential for the development and maintenance of dopaminergic neurons in the brain.
The general strategy to identify protein-metabolite interactions begins with the
recombinant expression and purification of the Nurr1 LBD (residues 328-598) with an N-terminal
His6 tag in Escherichia coli BL21(DE3) cells. To identify molecules that bind specifically to the
31
LBD it is immobilized on a metal ion affinity chromatography (IMAC) Sepharose 6 Fast Flow
resin, where it is incubated with a pool of candidate lipids extracted from wildtype mouse brain.
In this experiment, incubation of the resin in the absence of protein allows us to control for
nonspecific binding of lipid to the solid support. After incubation the extract is filtered, the beads
and protein are washed and the nuclear receptor is eluted from the resin. Eluted samples are
then analyzed using an untargeted liquid-chromatography-mass spectrometry (LC-MS) based
metabolomics platform that allows for the identification of lipids that are enriched in the protein
containing sample versus the controls.
This system requires that use of internal standards to assist in the calculation of fold
changes between metabolites in the sample sets 26-28. Metabolite profiles, the LC-MS
chromatograms from each sample, are compared using a software program called XCMS that
aligns the corresponding peaks in each sample and calculates their intensities by integrating the
area under the curves 29. The differences in ion intensities between sample peaks are ranked by
statistical significance (Student’s t-test) and assigned a fold change value that is normalized to
the internal standards 26-29. Finally, we will identify the structure of enriched ions by using
accurate mass (obtained during our standard MS experiments) and searching metabolite
databases, such as METLIN, PubChem, or the lipid MAPS databases, for metabolites with
similar molecular formulas 28.
32
Figure 2.2 A liquid chromatography-mass spectrometry (LC-MS)-based metabolomics
approach for characterizing endogenous nuclear receptor (NR) ligands. In the first step,
metabolites isolated from cells and tissues are incubated with the ligand-binding domain (LBD)
of an NR that has been immobilized onto a solid support (left). During the incubation any
endogenous ligands can bind to the NR and form a protein-metabolite complex (middle).
Unbound metabolites are then washed away and the nuclear receptor-ligand complex is eluted
from the resin. NR-bound metabolites are identified by comparing the LC-MS chromatograms
from the nuclear receptor sample to control sample using the program XCMS (right).
From the metabolomics assay I found that the Nurr1 LBD enriched polyunsaturated fatty
acids (PUFAs) (p-value < 0.05 and fold-change > 2) in comparison to the no-protein resin
control sample (Table 1). To be confident that we have identified endogenous ligands of Nurr1,
the candidates must bind with physiologically relevant dissociation constants (nM to uM range)30
to the receptor and be capable of regulating LBD dependent transcription. The secondary
biochemical assays that were perform to characterize the lipid-protein interaction were circular
dichroism (CD), which was used to measure conformational changes induced by lipid binding 25
(Figure 3) and an intrinsic tryptophan fluorescent assay, which was used to monitor saturation
binding (Figure 5)31. Additionally, the intrinsic tryptophan fluorescent assay was used to screen
prostaglandins (Figure 4) for their ability to bind the Nurr1 LBD as precedence for their ability to
33
regulate nuclear receptor function, particularly that of members of the NR4A family has already
been established20.
Enriched Lipids Fold Change
Docosapentaenoic acid (DPA, C22:5) 10.1
Docosahexaenoic acid (DHA, C22:6) 7.7
Arachidonic Acid (AA, C20:4) 7.1
Oleic acid (C18:1) 7.1
Linoleic (C18:2) 5.3
No Enrichment (Controls) Fold Change
Palmitic acid (PA, C16:0) 1.2
Stearic (C18:0) 1.2
Myristic (C14:0) 1.1
Table 2.1 Negative mode ions that are enriched by Nurr1-LBD greater than four-fold above
the resin control across three separate experiments. Polyunsaturated fatty acids (PUFAs) are
enriched, while saturated fatty acids are not. Positive mode analysis of samples did not reveal a
consistently enriched set of ions all three data sets.
Quenching of intrinsic tryptophan (Trp) fluorescence can be used to measure candidate
ligand binding. Excitation of Trp a 280nm will produce an emission at 330 nm when the residue
is buried (hydropobic environment) and an emission at 350 nm when the residue is solvent
accessible (polar environment). One caveat of this strategy is binding events with no impact on
the local environmental of Trp residues will not be identified, allowing for the occurrence of false
34
positives. The Nurr1 LBD (2 uM) was incubated with candidate ligands (50 um) in a screen of
saturated fatty acids, PUFAs and Prostaglandins (Figure 4). The fluorescence spectra is
quenched upon treatment with the unsaturated fatty acids Oleic (18:1), Arachidonic (20:4) and
Docosahexaenoic (22:6) as well as with the Prostaglandin B2, while remaining relatively
unchanged by the addition of saturated fatty acids and other prostaglandins. Furthermore,
titration assays showed that the PUFAs and PGB2 were able to saturate binding (Figure 5).
Indicating that the PUFAs and prostaglandins have the potential to be bona fide Nurr1 ligands.
To confirm the ability of the candidate ligands to modulate Nurr1 function, a cell based
luciferase reporter assay was used to measure the regulation of downstream transcriptional
activity in the presence of each candidate ligand. PUFAs and PGs did not have a significant
impact on transcriptional activation on their own. However, treatment of cells with a
benzimidazole activator (AROZ)24 followed by treatment with the candidate ligands identified
prostaglandins PGA2, PGB2, PGD2, and PGE2 as inverse agonists. PUFAs had no significant
impact on Nurr1 LBD dependent transcriptional activity, but there could be a variety of reasons
for this, such as their metabolism in these cell lines. The identification of PGs as inverse
agonists of Nurr1 is a novel finding, and would suggested increased inflammation would reduce
dopamine production, which is consistent with the implication of prostaglandin signaling in the
development of Parkinson’s Disease32.
35
Figure 2.3 Circular Dichroism of Nurr1-LBD and candidate ligands
Circular Dichrosim spectra of Nurr1-LBD (5uM) after incubation with candidate ligands (50 uM)
demonstrates that a variety of lipids can shift the secondary structure of the protein.
-4.00E+06
-3.50E+06
-3.00E+06
-2.50E+06
-2.00E+06
-1.50E+06
-1.00E+06
-5.00E+05
0.00E+00
204 209 214 219 224 229 234
Mo
lecu
lar
Ellip
tici
ty
Wavelength (nm)
Nurr1
Nurr1 + PA
Nurr1 + AA
Nurr1 + PGB2
Nurr1 + DHA
Nurr1 + AROZ
Nurr1 + PGA2
Nurr1 + Oleic
Nurr1 + CSNB
36
Figure 2.4 Intrinsic tryptophan fluorescence screen for lipid binding by Nurr1-LBD
The Nurr1-LBD was excited at 280 nM and its fluorescence monitored between 300-450 nM in
the presence of 25 molar equivalents of candidate ligand. The fluorescence spectra is lowered
upon treatment with the polyunsaturated fatty acids Oleic (18:1), Arachidonic (20:4) and
Docosahexaenoic (22:6) as well as with the Prostaglandin B2, while remaining relatively
unchanged by the addition of saturated fatty acids and other prostaglandins.
600
800
1000
1200
1400
1600
1800
2000
2200
2400
300 320 340 360 380
Fluorescence Emission (RFU)
Emission Wavelenght (nm)
DMSOControlPalmitic
20-OH-PGF2a
Oleic
TXB2
Arachidonic
PGE2
DHA
19R-OHPGE1
19R-OH-PGF2aPGD2
PGE1
PGF2B
37
Figure 2.5 Saturation binding curves using intrinsic tryptophan fluorescence
Ligand-binding curves for palmitic acid (PA), arachidonic acid (AA), oleic acid, prostaglandin B2
(PGB2), prostaglandin A2 (PGA2) and prostaglandin E2 (PGE2) were constructed by plotting the
change in fluorescence (relative to 0μM lipid) at the maximum emission wavelength (332 nM)
versus ligand concentration. With increasing concentrations of AA and Oleic acid (Kd ~33 μM)
and PGB2 (Kd ~105 μM) you see a saturating fluorescence response, while there is relatively
no change for PA of PGA2.
2.3 Conclusions
The PUFAs and PGs identified here are the first endogenous lipids identified to have a
regulatory impact on Nurr1 function. This finding demonstrates the effectiveness and value of
using an untargeted metabolomics approach to discover novel small molecule–protein
interactions with bioactive properties. The fact that PGs, most specifically PGD2 and PGE2,
have been implicated in the neuroinflammatory pathway contributing to the progression of
Parkinson’s Disease, positions this work to inform future research in targeting that pathway for
therapeutic development. Additionally, future structural studies will be important for the
identification and description of the NR4A unique mechanism of ligand-dependent
-200
0
200
400
600
800
1000
1200
0 50 100 150 200 250 300
-ΔF
at e
mis
sio
n 3
32
nm
(R
FU)
Lipid concentration (µM)
Palmitic
Arachidonic
Oleic
PGB2
PGA2
PGE2
38
transactivation. This piece of work has deorphanized Nurr1 and will hopefully serve as a starting
point for developing novel therapeutics that target the activity of this receptors for the treatment
of Parkinson’s disease.
2.4 Methods
Recombinant Nurr1LBD Expression (His6-Nurr1LBD) and Purification. Nurr1 LBD
(residues 328-598) with an N-terminal His6 tag was synthesized into the PJexpress411 vector
by DNA2.0. 1-2L cultures of Escherichia coli BL21(DE3) cells that had been transformed with
PJexpress411-His6-Nurr1LBD were grown with shaking in 2YT broth plus 50 µg/mL kanamycin
until mid-log phase, then induced with 1mM IPTG for 4 hours. Cells were harvested by
centrifugation (10 min at 10,000g) and stored at -80ºC until purification.
For purification of His6-Nurr1LBD protein, ≤2L cell pellets were resuspended in 35 mL
lysis buffer (20 mM Tris-HCl pH 7.9, 100 mM NaCl, 20 mM imidazole, 1% TritonX-100) and
were lysed by sonication at 4ºC. Lysate was cleared by centrifugation at 10,000g for 15 min at
4ºC. Soluble fraction was then loaded onto pre-equilibrated with lysis buffer nickel column
(IMAC Sepharose 6 Fast Flow Resin from GE Heathcare). Column was washed with 50 mL
lysis buffer and 100 mL was buffer (20 mM Tris-HCl pH 7.9, 100 mM NaCl, 20 mM imidazole),
before application of 30 mL elution buffer (20 mM Tris-HCl pH 7.9, 100 mM NaCl, 500 mM
imidazole). Eluate was concentrated using 10 kDa MWCO filter (Amicon). The protein was
further purified by Superdex 200 10/300 GL column (GE Healthcare) in SEC buffer (20 mM
Tris-HCl pH 7.9, 100 mM NaCl).
Tissue Extraction. An 8 mL solution of 2:1:1 CHCl3: MeOH: H2O was prepared for the
extraction of 1 frozen mouse brain (Pel-freez Biologicals) in a 15-mL dounce tissue grinder.
Sample was homogenized once ice until homogeneity was reached. Extract was then
transferred to glass vials for centrifugation at 2,500 g for 20 minutes to separate organic and
39
aqueous layers. Organic (bottom) layer was removed and concentrated under stream of
nitrogen gas. Extract was suspended in 200 uL of DMSO for use in enrichment experiments.
Stored at -80C.
Ligand enrichment experiments with His6-Nurr77LBD. A 10-μL suspension of IMAC
Sepharose 6 Fast Flow resin (GE Healthcare) was added to a 0.8 mL centrifuge column (Pierce
Scientific #89868) and charged with Ni2+ ions. The resins were washed with water (500μL and
then 2×100μL) and equilibrated equilibration with 3×200 μL of SEC buffer (20 mM Tris-HCl pH
7.9, 100 mM NaCl). Subsequently, the charged resins were incubated with either (i) 200 μL of
25μM His6-Nurr1LBD solution (experiment) or (ii) 200 μL protein SEC buffer (control). After 2 h
incubation at 4 °C, the unbound protein was separated from the resins by centrifugation, and the
resins were washed with 20 mM imidazole buffer (3× 200 μL). The lipid mixture (200 μL) was
then prepared as a solution in protein buffer containing 4% (v/v) DMSO (i.e., the mixture of 8 μL
lipid extracts in DMSO (or DMSO for no lipid control), and 192 μL protein buffer). After the resins
were incubated with the lipid mixture for 1 h at room temperature, the lipid mixture was removed
by centrifugation, and the resins were washed again for the last time with 20 mM imidazole
buffer (3×200 μL). In the last step, the elution of the protein or any metabolite-bound protein was
accomplished by incubating the resins with 100 μL of elution buffer (20 mM Tris-HCl pH 7.9, 100
mM NaCl, 500 mM imidazole) for 5 min prior to centrifugation. This step was repeated three
times. The elution fractions were combined, and the sample was stored at -80 °C until it was
analyzed by LC-MS.
LC-MS analysis of eluates from ligand enrichment experiment. LC-MS analysis was
performed using an Agilent 6220 LC-ESI-TOF instrument. For the LC analysis in the negative
mode, a Gemini (Phenomenex) C18 column (5 µm, 4.6 mm x 50 mm) and precolumn (C18, 3.5
µm, 2mm x 20mm) were used. Mobile phase A was a 95/5 water/methanol solution and mobile
40
phase B was a 60/35/5 isopropanol/methanol/water solution. Both mobile phase A and B were
supplemented with 0.1% ammonium hydroxide as a solvent modifier. The flow rate was set to
0.5 mL/min throughout the duration of the gradient. The gradient began at 0% B for 12 minutes
(first 10 minutes directed to waste) and then linearly increased to 100% B over the course of 40
min, followed by an isocratic gradient of 100% B for 6 min before equilibration to 0% B for 7min.
For LC analysis in the positive mode, a Luna (Phenomenex) C5 column (5 µm, 4.6 mm x
50 mm) and precolumn (C4, 3.5 µm, 2mm x 20mm) was used. Mobile phases A and B and
gradient remained the same as used in negative mode, except 0.1% formic acid and 5 mM
ammonium formate were used as solvent modifiers. The capillary voltage was set to 4.0 kV and
fragmentor voltage to 100V. The drying gas temperature was 350ºC and flow rate was 10L/min,
with the nebulizer pressure at 45 psi. Data was collected in both centroid and profile modes
using a mass range of 100-1500 Da. Each run was performed using 80 µL injections of eluates
from the ligand enrichment experiments and 45 µL for lipid mixtures.
LC-MS data analysis. Total ion chromatograms of eluates from the two sample sets
(N=3) of His6-Nurr1LBD + lipids or no protein resin control +lipids was collected. Two step
analyses was preformed, beginning with automated data analysis by XCMS followed by manual
statistical analysis, confirmation and filtering of XCMS output files. To identify metabolites
enriched by His6-Nurr1LBD the following parameters were used to filter XCMS output: fold
changes ≥ 2, statistical signifigance (p < 0.05), and minimum MSII of 10,000 in samples of His6-
Nurr1LBD + lipids. Visual inspection of EICs and elimination of isotopic peaks followed. Finally,
enriched lipids were confirmed to be present in applied lipid mixture.
Circular Dichroism (CD) Spectroscopy. CD spectroscopy was performed on a Jasco
J-710 spectropolarimeter. A chilled 200 uL mixture prepared containing 5 uM His6-Nurr1LBD
(20 mM Tris-HCl pH 7.9, 100 mM NaCl) and 50 µM of candidate ligand in ethanol (or equivalent
41
volume of pure ethanol for control), with the ethanol concentration not to exceed 5% (v/v). The
sample was then transferred to a quartz glass cuvette with 1-mm path length and scanned in
quadruplicate at 20ºC across the wavelengths of 260 nm to 190 nm. To obtain the final CD
spectrum, the raw data was subtracted i.e. protein containing sample minus buffer control,
smoothed using Savitzky-Golay method with the convolution width of 5 and calculated for molar
ellipticity values.
His6-Nurr1LBD intrinsic tryptophan fluorescence binding assay. In a 96 well
standard, opaque plate 2 µM His6-Nurr1LBD protein was mixed with 50 µM candidate ligand
(DMSO ≤5% v/v) in protein buffer (20 mM Tris-HCl pH 7.9, 100 mM NaCl). Data was collected
on a SpectraMax M5 Microplate Reader using an excitation wavelength of 280 nm, with
emission wavelength monitored between 300 to 450 nm, using a step size of 1 nm. Additional
settings: PMT sensitivity set to high, no cutoff selected, autocalibrate turned on, automix turned
off, and precision set to 14.
Transient Transfection and Reporter Analysis. To quantify Nurr1 transcriptional
activity, CV1 cells or HEK293 cells in 48-well plates were transfected with 100ng/well NBRE-
luciferase or NurRE-luciferase reporter, 50ng/well Nurr1, together with 50ng/well CMV--gal
reporter (as internal control for transfection efficiency). NurRE-luc and Nurr1 plasmids were
generously provided by Dr. Orla Conneely (Baylor College of Medicine). NBRE-luc plasmid was
generously provided by Dr. David Mangelsdorf (UT Southwestern). All transfection was
performed using FuGENE HD (Roche) (n=3) and repeated for at least three times. The cells
were treated with each compound or vehicle control 24 hrs after transfection. Reporter assays
were conducted 48 hrs after transfection, and luciferase activity was normalized by -gal
activity.
42
2.5 References
1. Huang, P., Chandra, V. & Rastinejad, F. Structural Overview of the Nuclear Receptor
Superfamily: Insights into Physiology and Therapeutics. Annual Review of Physiology
72, 247-272.
2. McEwan, I.J. Nuclear Receptors: One Big Family, in The Nuclear Receptor Superfamily,
Vol. 505 3-18 (Humana Press, 2009).
3. Sonoda, J., Pei, L. & Evans, R.M. Nuclear receptors: Decoding metabolic disease. FEBS
Letters 582, 2-9 (2008).
4. Chawla, A., Repa, J.J., Evans, R.M. & Mangelsdorf, D.J. Nuclear receptors and lipid
physiology: opening the X-files. Science 294, 1866-1870 (2001).
5. Sladek, F.M. What are nuclear receptor ligands? Molecular and Cellular Endocrinology
334, 3-13 (2011).
6. Nagy, L. & Schwabe, J.W.R. Mechanism of the nuclear receptor molecular switch.
Trends in Biochemical Sciences 29, 317-324 (2004).
7. Lonard, D.M., Lanz, R.B. & O'Malley, B.W. Nuclear receptor coregulators and human
disease. Endocr Rev 28, 575-587 (2007).
8. Thakur, M.K. & Paramanik, V. Role of steroid hormone coregulators in health and
disease. Horm Res 71, 194-200 (2009).
9. Rosenfeld, M.G., Lunyak, V.V. & Glass, C.K. Sensors and signals: a
coactivator/corepressor/epigenetic code for integrating signal-dependent programs of
transcriptional response. Genes & Development 20, 1405-1428 (2006).
10. Wang, Z. et al. Structure and function of Nurr1 identifies a class of ligand-independent
nuclear receptors. Nature 423, 555-560 (2003).
11. Pearen, M.A. & Muscat, G.E.O. Minireview: Nuclear Hormone Receptor 4A Signaling:
Implications for Metabolic Disease. Mol Endocrinol 24, 1891-1903 (2010).
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12. Muscat, M.A.M.a.G.E.O. The NR4A subgroup: immediate early response genes with
pleiotropic physiological roles. Nuclear Receptor Signaling 4 (2006).
13. Pei, L. et al. NR4A orphan nuclear receptors are transcriptional regulators of hepatic
glucose metabolism. Nat Med 12, 1048-1055 (2006).
14. Chao, L.C. et al. Insulin resistance and altered systemic glucose metabolism in mice
lacking Nur77. Diabetes 58, 2788-2796 (2009).
15. Le, W.D. et al. Mutations in NR4A2 associated with familial Parkinson disease. Nat
Genet 33, 85-89 (2003).
16. Hawk, J.D. & Abel, T. The role of NR4A transcription factors in memory formation. Brain
Res Bull 85, 21-29 (2011).
17. Flaig, R., Greschik, H., Peluso-Iltis, C. & Moras, D. Structural Basis for the Cell-specific
Activities of the NGFI-B and the Nurr1 Ligand-binding Domain. Journal of Biological
Chemistry 280, 19250-19258 (2005).
18. Codina, A. et al. Identification of a novel co-regulator interaction surface on the ligand
binding domain of Nurr1 using NMR footprinting. J Biol Chem 279, 53338-53345 (2004).
19. Volakakis, N., Malewicz, M., Kadkhodai, B., Perlmann, T. & Benoit, G. Characterization
of the Nurr1 ligand-binding domain co-activator interaction surface. Journal of molecular
endocrinology 37, 317-326 (2006).
20. Kagaya, S. et al. Prostaglandin A(2) acts as a transactivator for NOR1 (NR4A3) within
the nuclear receptor superfamily. Biol Pharm Bull 28, 1603-1607 (2005).
21. Zhan, Y. et al. Cytosporone B is an agonist for nuclear orphan receptor Nur77. Nat
Chem Biol 4, 548-556 (2008).
22. Chintharlapalli, S. et al. Activation of Nur77 by Selected 1,1-Bis(3′-indolyl)-1-(p-
substituted phenyl)methanes Induces Apoptosis through Nuclear Pathways. Journal of
Biological Chemistry 280, 24903-24914 (2005).
44
23. Dubois, C., Hengerer, B. & Mattes, H. Identification of a potent agonist of the orphan
nuclear receptor Nurr1. ChemMedChem 1, 955-958 (2006).
24. Hintermann, S. et al. Identification of a series of highly potent activators of the Nurr1
signaling pathway. Bioorg Med Chem Lett 17, 193-196 (2007).
25. Vinayavekhin, N. & Saghatelian, A. Discovery of a Protein–Metabolite Interaction
between Unsaturated Fatty Acids and the Nuclear Receptor Nur77 Using a
Metabolomics Approach. J Am Chem Soc 133, 17168-17171 (2011).
26. Tagore, R., Thomas, H.R., Homan, E.A., Munawar, A. & Saghatelian, A. A global
metabolite profiling approach to identify protein-metabolite interactions. J Am Chem Soc
130, 14111-14113 (2008).
27. Kim, Y.G., Lou, A.C. & Saghatelian, A. A metabolomics strategy for detecting protein-
metabolite interactions to identify natural nuclear receptor ligands. Mol Biosyst 7, 1046-
1049 (2011).
28. Vinayavekhin, N. & Saghatelian, A. Regulation of alkyl-dihydrothiazole-carboxylates
(ATCs) by iron and the pyochelin gene cluster in Pseudomonas aeruginosa. ACS Chem
Biol 4, 617-623 (2009).
29. Smith, C.A., Want, E.J., O'Maille, G., Abagyan, R. & Siuzdak, G. XCMS: processing
mass spectrometry data for metabolite profiling using nonlinear peak alignment,
matching, and identification. Anal Chem 78, 779-787 (2006).
30. Escriva, H., Delaunay, F. & Laudet, V. Ligand binding and nuclear receptor evolution.
BioEssays 22, 717-727 (2000).
31. Petrescu, A.D., Hertz, R., Bar-Tana, J., Schroeder, F. & Kier, A.B. Ligand Specificity and
Conformational Dependence of the Hepatic Nuclear Factor-4α (HNF-4α). Journal of
Biological Chemistry 277, 23988-23999 (2002).
45
32. Lima, I.V.d.A., Bastos, L.F.S., Limborço-Filho, M., Fiebich, B.L. & de Oliveira, A.C.P.
Role of Prostaglandins in Neuroinflammatory and Neurodegenerative Diseases.
Mediators of Inflammation 2012, 13 (2012).
46
Chapter 3
Anti-Diabetic Activity of Insulin-Degrading Enzyme Inhibitors Mediated by
Multiple Hormones
This chapter was adapted from:
Maianti, JP, McFedries, A, et. al.. Anti-Diabetic Activity of Insulin-Degrading Enzyme Inhibitors
Mediated by Multiple Hormones. Nature. Accepted 2014.
47
3.1 Introduction
The dynamic interplay between the production and proteolytic degradation of peptide
hormones is a key mechanism underlying the regulation of human metabolism. Inhibition of the
peptidases and proteases that degrade these hormones can elevate their effective
concentrations and augment signaling. In some cases, the resulting insights can lead to the
development of novel therapeutics1. Dipeptidyl peptidase 4 (DPP4) inhibitors, for example, are
anti-diabetic drugs that increase the concentration of the insulin-stimulating hormone glucagon-
like peptide 1 (GLP-1), resulting in elevated insulin concentrations and lower blood glucose
levels2. Researchers have speculated for at least six decades that insulin signaling could also
be augmented to improve glucose tolerance by inhibiting its degradation3,4. The zinc
metalloprotease insulin-degrading enzyme (IDE) is thought to be the primary enzyme
responsible for inactivation of insulin in the liver, kidneys, and target tissues3,4. Recently,
genome-wide association studies have identified predisposing and protective variants of the IDE
locus linked to type-2 diabetes (T2D)5-9, suggesting a functional connection between IDE and
glucose regulation in humans.
Based on the known biochemistry of IDE, inhibition of this enzyme is expected to elevate
insulin levels and augment the response to glucose3,4. While mice lacking a functional IDE gene
(IDE–/– mice) have elevated insulin levels, counterintuitively these animals exhibit impaired,
rather than improved, glucose tolerance10,11. Physiological studies with IDE–/– mice concluded
that chronic elevation of insulin in these animals results in a compensatory lowering of insulin
receptor expression levels, which leads to impaired glucose clearance following a glucose
load10,11. This model raises the possibility that in the absence of such compensatory effects,
acute inhibition of IDE may lead to improved physiological glucose tolerance.
Acute inhibition of enzymes is typically achieved through the use of small-molecule
inhibitors, but the only previously reported IDE inhibitors are analogs of the linear peptide
48
mimetic Ii1 (Fig. 3.1)12,13, which is highly unstable in vivo11. These compounds derive potency
from a zinc-chelating hydroxamic acid group, which has the potential to interact strongly with
other metalloproteases and metal-binding proteins14. These observations highlight the need for
a selective small-molecule IDE inhibitor to characterize the biological functions and therapeutic
relevance of this enzyme in vivo15,16, uncoupled from confounding physiological adaptations that
arise in IDE knock-out mice10,11. In this study we set out to discover potent and selective small-
molecule IDE inhibitors that are active in vivo, and to use these compounds to reveal the
physiological consequences of IDE inhibition.
3.2 Potent and selective IDE inhibitors
Ralph Kleiner and Juan Pablo Mainanti in the Liu lab led the discovery of small-molecule
modulators of IDE, we performed in vitro selections on a previously described DNA-templated
library of 13,824 synthetic macrocycles17,18 for the ability to bind immobilized mouse IDE (Fig.
A3.1). This library previously yielded highly selective Src kinase inhibitors,19,20 and its unbiased
design features and structural diversity suggested it may also contain ligands for other classes
of proteins. Since each macrocycle in this library is attached to a unique DNA oligonucleotide
that can be used to identify the structures of IDE-binding macrocycles18,19, we used high-
throughput DNA sequencing revealed the macrocycle-encoding DNA templates that were
enriched following in vitro selection. Two independent IDE selection experiments, resulted in
the identification of six putative IDE-binding macrocycles that share common structural features
(Fig. 3a, Fig. A3.1).
49
Figure 3.1 Discovery of potent and highly selective macrocyclic IDE inhibitors from the in
vitro selection of a DNA-templated macrocycle library. a, Structure of the most potent hit
from the IDE selection (6b) and a summary of the requirements for IDE inhibition revealed by
the synthesis and evaluation of 6b analogs. b, IDE inhibition potency of selection hits 1b to 6b
and 30 structurally related analogs in which the linker, scaffold, and three building blocks were
systematically varied. c, Structure of physiologically active IDE inhibitor 6bK. d, Structure of
the inactive diastereomer bisepi-6bK. e, Structure of the previously reported substrate-mimetic
hydroxamic acid inhibitor Ii112. (F) Selectivity analysis of macrocycle 6bK reveals > 1,000-fold
selectivity for IDE ( , IC50 = 50 nM) over all other metalloproteases tested. g, Inhibitor Ii112
inhibits IDE ( IDE, IC50 = 0.6 nM), and also thimet oligopeptidase ( THOP, IC50 = 6 nM) and
neurolysin ( NLN, IC50 = 185 nM), but not neprilysin ( NEP), matrix metalloprotease 1
( MMP1), or angiotensin converting-enzyme ( ACE). Human IDE shares 95 % primary
sequence homology with mouse IDE24, and both are inhibited by the macrocycles used in this
study with similar potency (Fig. A2.2).
0.001 0.01 0.1 1 10 100
6bK concentration (µM)
(L-alanine) 15
(D-alanine) 16
(2-Me-alanine) 17
(N-Me-alanine) 18
(serine) 19
(glycine) 20
(lysine) 6bK
(glutamate) 21
(methionine sulfoxide) 22
(selenomethionine) 23
(phenylalanine) 24
(none/skipped) 25
(D-Lys amide) 26
(L-ornithine amide) 27
(L-Lys carboxylate) 28
(L-Lys, αN-ethylamide) 29
(L-Lys, biotin tag) 30
(L-Lys, fluorescein tag) 31
inhibitor potency, IDE IC50 (M)
(trans) 1b
(trans) 2b
(trans) 3b
(trans) 4b
(trans) 5b
(trans) 6b
(cis) 6a
(saturated) 6c
(D-4-benzyl-Phe) 7
(D-phenylalanine) 8
(D-4-tertBu-Phe) 9
(D-4-phenyl-Phe) 10
(phenylalanine) 11
(norisoleucine) 12
(leucine) 13
(alanine) 14
inhibitor potency, IDE IC50 (M)
building block A
selection hits
diamide linker
building block B
building block C
scaffold block D
6bK
IC50 = 50 nM bisepi-6bK
IC50 > 200 µM
c d
a b
0%
20%
40%
60%
80%
100%
en
zym
e in
hib
itio
n
6bK concentration (µM)
NLN
THOP
NEP
MMP1
ACE
f
0%
20%
40%
60%
80%
100%
0.00001 0.0001 0.001 0.01 0.1 1 10 100
en
zym
e inh
ibitio
n
Ii1 concentration (µM)
NLN
THOP
NEP
MMP1
ACE
e
Ii1
hydroxamic acid (red group)
linear tetrapeptide IDE inhibitor
g
IDE IDE
6b (reference)
IC50 = 60 nM
10-8 10-6 10-5 10-4 10-3 10-7 10-8 10-6 10-510-4 10-3 10-7
HN
NH
HN
NH2
O
O O-
O
O
NH
NH3+HN
O
NH
O
HO
NH
50
We synthesized these six macrocycles without their oligonucleotide templates and without
the 5-atom macrocycle-DNA linker using solid- and solution-phase synthesis as either of two
possible cis- or trans-alkene stereoisomers18,19 (Fig. A3.1). Biochemical assays revealed that
four of the six trans-macrocycles assayed were bona fide inhibitors of IDE with IC50 ≤ 1.5 µM
(Fig. A3.1). The most active inhibitor among the library members enriched in the selection, 20-
membered macrocycle 6b (Fig. 3.1a), potently inhibited human IDE (IC50 = 60 nM). The ability
of 6b to inhibit IDE proteolytic activity in vitro was confirmed by three complementary assays
using a fluorogenic peptide, an insulin immunoassay, and a calcitonin-gene related peptide LC-
MS assay (Fig. A3.2)21.
We synthesized and biochemically assayed 30 analogs of 6b in which each building block
was systematically varied to elucidate structure-activity relationships of these inhibitors (Fig.
3.1b). These studies revealed the structural requirements required for potent IDE inhibition by
this new class of molecules, including a trans-fused 20-membered macrocycle, the
stereochemistry of the macrocycle substituents, and the size, shape, and hydrophobicity of the
A and B building blocks (Fig. 3.1a). In contrast to the strict requirements at positions A and B,
different building blocks were tolerated at position C (Fig. 3.1b). Based on these results, we
identified the inhibitor 6bK (IC50 = 50 nM, Fig. 3.1c) as an ideal candidate for in vivo studies
because it exhibits enhanced water solubility relative to 6b, and can be readily synthesized on
gram scale16.
Because selectivity is a crucial feature of effective probes to elucidate physiological
functions16, we next characterized the protease inhibition selectivity of 6bK. This inhibitor
exhibited ≥ 1,000-fold selectivity in vitro for IDE over all other metalloproteases tested: thimet
oligopeptidase (THOP), neurolysin (NLN), neprilysin, matrix metalloprotease 1, and angiotensin
converting-enzyme (Fig. 2.1f). In contrast, the previously reported substrate mimetic
hydroxamic acid inhibitor Ii112 (Fig. 2.1e) is not as selective and it potently inhibits IDE (IC50 =
0.6 nM), THOP (IC50 = 6 nM), and NLN (IC50 = 185 nM) (Fig. 3.1g). The remarkable selectivity
51
of 6bK, in contrast with the known promiscuity of some active site-directed metalloprotease
inhibitors14, led us to speculate that the macrocycle engages a binding site distinct from the
enzyme’s catalytic site. This hypothesis was supported by double-inhibitor kinetic assays that
revealed synergistic, rather than competitive, inhibition by macrocycle 6b and substrate mimetic
Ii1 (Fig. A2.2).
3.3 Structural basis of IDE inhibition
In collaboration with Markus Selegur’s lab, Juan Pablo and Zach Foda determined the
molecular basis of IDE inhibition and selectivity by these macrocycles, we determined the X-ray
crystal structure of catalytically inactive cysteine-free human IDE-E111Q22 bound to 6b at 2.7 Å
resolution (Fig. 3.2, Fig. A3.3a). The enzyme adopted a closed conformation and its structure is
essentially identical to that of apo-IDE (PDB 3QZ2, RMSD = 0.257 Å). Macrocycle 6b occupies
a binding pocket at the interface of IDE domains 1 and 2 (Fig. 3.2a), and is positioned more
than 11 Å away from the zinc ion in the catalytic site (Figs. 3.2b and 3.2c). This distal binding
site is a unique structural feature of IDE compared to related metalloproteases23, and does not
overlap with the binding site of the substrate-mimetic inhibitor Ii112. The structure suggests that
by engaging this distal site, the macrocycle competes with substrate binding (Fig. A3.3) and
abrogates key interactions that are necessary to unfold peptide substrates for cleavage24-26 (Fig.
3.2d).
52
Figure 3.2 Structural basis of IDE inhibition by macrocycle 6b. a, X-ray co-crystal structure
of IDE bound to macrocyclic inhibitor 6b (2.7 Å resolution, pdb: 4LTE). IDE domains 1, 2, 3,
and 4 are colored green, blue, yellow, and red, respectively. Macrocycle 6b is represented as a
ball-and-stick model, and the catalytic zinc atom is represented as an orange sphere. b,
Electron density map (composite omit map contoured at 1σ) and model of IDE-bound
macrocycle 6b interacting with a 10 Å-deep hydrophobic pocket. c, Relative position of
macrocycle 6b bound 11 Å from the catalytic zinc atom. d, Overlay of the 6b model (surface
rendering) on the IDE:insulin co-crystal structure (pdb: 2WBY)26. e, Activity assays for wild-type
or mutant human IDE variants in the presence of 6bK. Mutagenesis of residues Ala479Leu ()
and Gly362Gln () hindered the inhibition potency of 6bK by > 600- and > 50-fold, respectively,
compared to that of wild-type human IDE ().
catalytic site
6b
6b 10 Å
catalytic site exo site 6b insulin
building-block A
building-block B
catalytic site
Ala479 Ala198 Trp199
Gly362 Phe202 6b
0%
20%
40%
60%
80%
100%
0.0001 0.001 0.01 0.1 1 10 100 1000
enzym
e inhib
itio
n
6bK concentration (µM)
hIDE WT
G362Q IDE
A479L IDE
a
d
c
b
e
11 Å
53
Because a section of the macrocycle was unresolved in the electronic density map, as
observed with other ligands co-crystallized within the IDE cavity,12 we sought to test the
relevance of our structural model of the macrocycle:IDE complex (Fig. A3.3) to macrocycle:IDE
binding in solution. We identified IDE mutations predicted by the structural model to impede 6b
binding (Fig. 3.2e), prepared the corresponding mutant IDE proteins, and measured their
abilities to be inhibited by 6b and 6bK. In addition, we also synthesized 6b analogs designed to
complement these mutations and rescue inhibitor potency (Fig. A3.4). Building block A (p-
benzoyl-phenylalanine in 6b) occupies a 10 Å-deep pocket in the crystal structure (Fig. 3.2b),
defined by residues Leu201, Gly205, Tyr302, Thr316, and Ala479. As predicted by the
structural model, mutation of Ala479 to leucine decreased the potency of inhibitors 6b and 6bK
more than 600-fold, consistent with a significant steric clash in the binding site between Leu479
and the distal benzoyl group in building block A (Fig. 3.2e). Replacement of the p-benzoyl-
phenylalanine building block with the smaller tert-butyl-phenylalanine, macrocycle 9, inhibited
A479L-IDE with equal potency as wild-type IDE, consistent with the ability of the smaller
macrocycle 9 to accommodate the added bulk of the leucine side chain (Fig. A3.4). Likewise,
building block B (cyclohexylalanine in 6b) makes contacts in the structure with the peptide
backbone of residues Val360, Gly361, and Gly362 located on the lateral β-strand 13 of IDE
domain 2. These residues are thought to assist in unfolding of large peptide substrates by
promoting cross-β-sheet interactions24-26. Mutation of Gly362 to glutamine decreased the
inhibition potencies of 6b and 6bK at least 50-fold compared to wild-type IDE (Fig. 3.2e). A
modified macrocycle (13) in which the cyclohexylalanine building block was replaced with a
smaller leucine residue inhibited G362Q IDE and wild-type IDE comparably, consistent with a
model in which the smaller B building block complemented the larger size of the glutamine side
chain (Fig. A3.4).
Together, these structural and biochemical studies provide strong evidence for the
proposed distal binding site of 6b and demonstrate the ability of the DNA-templated macrocycle
54
library to provide inhibitors that achieve unusual selectivity by targeting residues beyond the
catalytic site. IDE is the only homolog of the M16 clade of metalloproteases, which is
evolutionarily distinct from other zinc-dependent metalloprotease members and characterized
by an inverted zinc-binding motif23-26. This distinct phylogenetic origin, together with the unusual
binding mode of these macrocyclic inhibitors to IDE, may contribute to the unusual specificity of
6bK among proteases tested and encouraged us to explore the properties of 6bK in vivo.
3.4 Inhibition of IDE in vivo
Next we characterized the stability, physicochemical, and pharmacokinetic properties of
6bK. This macrocycle displayed significant stability during incubations with plasma and liver
microsome preparations (74 % and 78 % remaining after 1 h, respectively), suggesting that this
compound may be sufficiently stable in vivo to inhibit IDE activity. Plasma protein binding
assays indicated that ~6 % of 6bK remains unbound and potentially available to engage its
target at sites of insulin degradation, extracellularly or in early endosome compartments of
target tissues3,12. To measure plasma half-life in vivo, we treated mice by intraperitoneal (i.p.)
injection of 80 mg/kg 6bK using a formulation of sterile saline and Captisol, a β-cyclodextrin-
based agent used to improve solubilization and delivery27. Plasma and tissue concentrations of
6bK were measured using isotope dilution mass spectrometry (IDMS) (Fig. A3.5). Plasma
levels of 6bK were detectable 5 min post-injection, reached peak concentration (> 100 µM) at 60
min, and were maintained at a detectable level for at least 4 h (Fig. A3.5). This circulation time
is within the timescale for standard physiological experiments with live animals28,29. We
observed prompt biodistribution of 6bK into plasma, liver, kidney, and pancreatic tissues (Fig.
A3.5). We did not detect any 6bK in the brain, suggesting that this macrocycle may not inhibit
IDE within brain tissues, where IDE activity is needed for the clearance of β-amyloid peptides10.
Indeed, brain tissue levels of Aβ(40) and Aβ(42) peptides in mice injected with 6bK were
unchanged 2 h-post injection compared to vehicle-treated controls (Fig. A3.6), consistent with
55
the inability of 6bK to inhibit IDE in the brain. Collectively, these observations suggested the
viability of 6bK as a potential in vivo IDE inhibitor probe in peripheral tissues of mice16.
To evaluate the ability of 6bK to inhibit IDE activity in vivo, we subjected non-fasted mice
to insulin tolerance tests (ITT)29 following a single injection with 6bK (80 mg/kg) formulated in
Captisol27. The insulin injections were carried out 30 min post-injection, corresponding to the
time of highest 6bK concentration in plasma (approximately 100 µM, ~1000-fold the IC50 for
mouse IDE). Following a subcutaneous insulin injection, mice treated with 6bK experienced
lower hypoglycemia and higher insulin levels compared to vehicle controls (p < 0.01, Fig. A3.6
and Fig. 3.4b). In 1955, Mirsky used a similar ITT assay to suggest the feasibility of insulin
stabilization by injecting rats with preparations of an undefined endogenous IDE inhibitor crudely
fractionated from bovine livers (presumably a competitive substrate; see Appendix Table 1)30.
Our experiments with 6bK provide the first evidence that a well-defined, selective, and
physiologically stable pharmacological IDE inhibitor can augment the abundance and activity of
insulin in vivo. Testing the macrocycle at several doses established an effective dose of 6bK of
~2 mg/mouse i.p., representing 80 mg/kg for lean C57BL/6J mice (25 g), and 60 mg/kg for diet-
induced obese (DIO) mice (35-45 g). These inhibitor doses were well tolerated, did not produce
adverse reactions, or body weight loss (Fig. A3.6), and did not induce detectable behavioral
abnormalities.
3.5 Anti-diabetic activity of IDE inhibition during oral glucose administration
To determine the physiological consequences of acute IDE inhibition in vivo, we evaluated
glucose tolerance of mice treated with 6bK. We used two methods of glucose delivery, either
oral gavage or i.p. injection,28 and two different mouse models, lean or DIO mice31,32. These
four conditions were chosen to survey the role of IDE activity under a broad range of
endogenous insulin levels and insulin sensitivity28,31. Oral glucose administration, for example,
results in greater insulin secretion compared to injected glucose delivery (Fig. A3.7). Passage
56
of glucose through the gut causes the release of GLP-1, which strongly augments glucose-
dependent insulin secretion2,31. This phenomenon is referred to as the ‘incretin effect’ (Fig.
A3.7) and is magnified in DIO mice31. In addition, DIO mice display hyperinsulinemia and
insulin resistance compared to lean mice, enabling us to test the consequences of IDE inhibition
in a model that resembles early type-2 diabetes in humans32.
In all glucose tolerance experiments we included two control groups: vehicle alone, and
the inactive isomer16 bisepi-6bK (Fig. 3.1c), which is identical to 6bK in chemical composition
and bond connectivity, but has virtually no IDE inhibition activity (IC50 > 100 µM, Fig. 3.1c, see
also Fig. A2.8). As expected, administration of 6bK alone, without a glucose challenge, did not
significantly alter basal blood glucose or hormone levels compared to control treatments (Fig.
A3.8). We then examined the effect of 6bK on blood glucose levels during an oral glucose
tolerance test (OGTT). Lean or DIO mice were fasted overnight for these experiments, and
then treated with a single dose of 6bK, vehicle alone, or a matching dose of inactive bisepi-6bK.
After 30 minutes, glucose was administered by oral gavage.
Importantly, both lean and DIO mice treated with 6bK displayed significantly improved oral
glucose tolerance compared to vehicle or inactive bisepi-6bK control groups (Fig. 3.3 and Fig.
A3.9). Effects of similar magnitude on oral glucose tolerance in mice have been observed using
several known human anti-diabetic therapeutics33-36. The two control groups exhibited similar
blood glucose profiles, indicating that the observed effects of 6bK on glucose tolerance are lost
when the stereochemistry of 6bK is altered in a way that abolishes IDE inhibition.
To further test if the observed effects of 6bK are specific to its interaction with IDE, we
repeated these experiments using IDE–/– knockout mice10,11. Mice lacking IDE were unaffected
by 6bK treatment, and exhibited blood glucose responses indistinguishable to that of the
vehicle-treated cohort (Fig. A3.10). These results indicate that the effects of 6bK are dependent
on the presence of IDE.
57
Collectively, these observations support a model in which IDE regulates glucose-induced
insulin signaling, and therefore glucose tolerance, and demonstrate that acute IDE inhibition
improves post-prandial glucose control in lean and DIO mice (Fig. 3.3a and 3.3b). Together,
these results represent the first time that IDE inhibition has been shown to improve blood
glucose tolerance3,30.
58
Figure 3.3 Physiological consequences of acute IDE inhibition by 6bK on glucose
tolerance in lean and DIO mice. a and b, Oral glucose tolerance during acute IDE inhibition.
a, Male C57BL/6J lean (25 g) mice were treated with a single i.p. injection of IDE inhibitor 6bK
(, 80 mg/kg), inactive control bisepi-6bK (, 80 mg/kg), or vehicle alone () 30 min prior to
glucose gavage (3.0 g/kg). b, DIO mice (35-45 g) were treated with 6bK (, 60 mg/kg), and
inactive control bisepi-6bK (, 60 mg/kg) or vehicle alone () 30 min prior to glucose gavage
(3.0 g/kg). c and d, Glucose tolerance phenotypes after i.p. injection of glucose (1.5 g/kg) in
lean (c) and DIO (d) male mice treated with 6bK (), inactive bisepi-6bK (), or vehicle alone
(). Area under the curve (AUC) calculations are shown in Extended Data Fig. 9. All data
points and error bars represent mean ± SEM. Significance tests were performed using two-tail
Student’s t-test, and significance levels shown are p < 0.05 (*) or p < 0.01 (**) versus the
vehicle-only control group.
0
100
200
300
400
500
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
bisepi (60 mg/kg)
6bK (60 mg/kg)
Vehicle
*
Rx i.p.
glucose
**
** **
(n = 7-8)
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose gavage (3.0 g/kg)
bisepi (60 mg/kg)
6bK (60 mg/kg)
Vehicle
Rx
oral
glucose
** * * *
(n = 6-7)
blo
od
glu
co
se
(m
g/d
L)
blo
od
glu
co
se (
mg/d
L)
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose gavage (3.0 g/kg)
bisepi (80 mg/kg)
6bK (80 mg/kg)
Vehicle
Rx
oral
glucose
* *
*
(n = 6-7)
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
bisepi (80 mg/kg)
6bK (80 mg/kg)
Vehicle**
*
*
Rx
i.p.
glucose
(n = 5-6)
a b
c d
oral glucose, lean mice oral glucose, DIO mice
injected glucose, lean mice injected glucose, DIO mice
6bK
bisepi
6bK
bisepi
6bK
bisepi
6bK
bisepi
59
3.6 IDE inhibition during an injected glucose challenge leads to impaired glucose
tolerance
Prior work using IDE–/– mice characterized the effect of i.p. glucose injections, therefore we
repeated the above experiments with 6bK followed by i.p. injected glucose tolerance tests
(IPGTTs) to provide a more direct comparison with the knockout animal experiments10,11. In
contrast to the observed improvement in oral glucose tolerance upon 6bK treatment (Figs. 3.3a
and 3.3b), IDE inhibition with 6bK followed by a glucose injection (1.5 g/kg i.p.) resulted in
impaired glucose tolerance after 2 h in both lean and obese mice compared to vehicle alone or
bisepi-6bK-treated controls (Figs. 3.3c and 3.3d). These changes in the glucose response
profiles of lean mice treated with 6bK compared to vehicle controls resemble the reported
differences between IDE–/– and IDE+/+ mice during similar IPGTTs10,11. Moreover, DIO mice
treated with 6bK followed by glucose injection displayed a biphasic response in which glucose
levels are lower over the initial 30 minutes of the IPGTT, followed by a hyperglycemic “rebound”
starting 1 h after glucose injection (Fig. 3.3d). Both the suppression of peak glucose levels and
the magnitude of the hyperglycemic rebound were dependent on 6bK dose, and neither effect
was observed in cohorts treated with vehicle alone or inactive bisepi-6bK, indicating that the
impaired glucose tolerance during an IPGTT correlates with IDE activity (Fig. 3.3, and Fig.
A3.9).
Collectively, the results of the OGTTs and IPGTTs indicate that the route of glucose
administration impacts the physiological response of 6bK-treated animals in ways that cannot
be explained by a simple model in which IDE’s physiological role is only to degrade insulin.
Instead, the IPGTT results strongly suggest a role for IDE in regulating other glucose-regulating
peptide hormones in vivo.
60
3.7 IDE regulates multiple hormones in vivo
The biochemical properties of IDE and its substrate recognition mechanism23-25 enable this
enzyme to cleave a wide range of peptide substrates in vitro (Appendix 3 Table 1). Two
glucose-regulating hormones, beyond insulin, that are potential candidates for physiological
regulation by IDE during a glucose challenge are glucagon and amylin. Purified IDE has been
previously shown to cleave both peptides in vitro37-39, but neither hormone is known to be
regulated by IDE activity in vivo. Compared to insulin, glucagon is a modest in vitro IDE
substrate (KM = 3.5 µM for glucagon versus KM < 30 nM for insulin)37, although IDE is capable of
degrading glucagon at a comparable rate if present in sufficiently high concentrations (kcat = 38
min-1 for glucagon)38. Amylin is also a substrate for IDE in vitro (KM = ~0.3 µM)39. Other
proteases suggested to degrade glucagon include nardilysin, cathepsin B and D, in cells and in
vitro40,41, and neprilysin, which was shown to play a role in renal clearance of glucagon42.
However, none of these enzymes are known to regulate endogenous processing of hormones
or modulate blood glucose levels. To our knowledge, no proteases have been previously
shown to degrade amylin in vivo39.
To begin to probe the possibility that glucagon or amylin is regulated in vivo by IDE, we
measured the plasma levels of these hormones at 20 and 130 minutes post-glucose injection in
DIO mice treated with 6bK or vehicle alone during an IPGTT (Fig. 3.4a). Plasma collected 20
minutes post-glucose injection showed elevated insulin and amylin levels, but unchanged
glucagon levels, for the 6bK-treated cohort relative to the control group (Fig. 2.4a). During the
hyperglycemic rebound 130 min post-injection, glucagon levels for the 6bK group were strongly
elevated above 200 pg/mL, compared with 90 pg/mL glucagon in control mice (Fig. 3.4a).
Consistent with these elevated glucagon levels, expression of a gluconeogenesis transcriptional
marker, G6Pase, was elevated in the livers of 6bK-treated mice compared to control mice (Fig.
3.4a).
61
Figure 3.4 Acute IDE inhibition affects the abundance of multiple hormone substrates
and their corresponding effects on blood glucose levels. a, Plasma hormone
measurements at 20 and 135 minutes post-IPGTT (Fig. 3.3d) for DIO mice treated with 6bK ()
or vehicle alone (). RT-PCR analysis of DIO liver samples collected at 135 min post-IPGTT
reveals 50 % higher glucose-6-phosphatease (G6Pase) and 30 % lower phosphoenolpyruvate
carboxykinase (PEPCK) transcript levels for the 6bK-treated cohort () versus vehicle-only (V)
controls (). b to d, Blood glucose responses and abundance of injected hormones in lean
mice 30 min after treatment with 6bK (, 80 mg/kg) or vehicle alone (). b, Insulin s.c. (0.25
U/kg) after 5-hour fast. c, Amylin s.c. (250 µg/kg) after overnight fast. d, Glucagon s.c. (100
µg/kg) after overnight fast. Trunk blood was collected at the last time points for plasma
hormone measurements (insets). All data points and error bars represent mean ± SEM.
Significance tests were performed using two-tail Student’s t-test, and significance levels shown
are p < 0.05 (*) or p < 0.01 (**) versus the vehicle-only control group.
0
2
4
6
8
10
12
0.0
0.1
0.2
0.3
0
0.2
0.4
0
50
100
150
200
-60 -30 0 30
6bK (80 mg/kg)
Vehicle
Rx glucagon
(n = 7) **
**
0
50
100
150
200
-60 -30 0 30 60
6bK (80 mg/kg)
Vehicle
Rx amylin
** **
(n = 8-9)
0
50
100
150
200
-60 -30 0 30 60
6bK (80 mg/kg)
Vehicle
Rx insulin
**
*
0
1
2
3
4
insu
lin (µ
IU/m
L) (n = 11-12)
min. post-insulin injection (0.25 U/kg) min. post-glucagon inj. (100 µg/kg) min. post-amylin injection (250 µg/kg)
blo
od
glu
co
se (
mg/d
L)
0
1
2
glu
cag
on
(n
g/m
L)
0
5
10
15
20
25
b d
**
- +
**
- +
**
- +
am
ylin
(n
g/m
L)
c insulin tolerance test amylin challenge glucagon challenge
6bK 6bK
6bK
DIO mice hormone measurements and gluconeogenesis transcriptional markers post-glucose injection (IPGTT) a
0.0
1.0
2.0
3.0 ** **
PEPCK G6Pase
rela
tive
expre
ssio
n
V 6bK V 6bK
insulin
(ng/m
L)
glu
ca
go
n (
ng/m
L)
am
ylin
(ng/m
L)
20 min 135 min
** ** **
*
V 6bK V 6bK
20 min 135 min
V 6bK V 6bK
20 min 135 min
V 6bK V 6bK
135 min
62
Because hormone abundance measurements can be difficult to interpret during
fluctuations in blood glucose that in turn affect pancreatic hormone secretion, we performed
additional studies to confirm the relationship between IDE activity and glucagon and amylin
levels in vivo. To more directly establish the effect of IDE inhibition on the clearance of insulin,
amylin, and glucagon in vivo, we injected each of these three hormones into lean mice 30 min
after treatment with 6bK or vehicle alone (Figs. 3.4b to 3.4d). The 6bK-treated cohorts exhibited
significantly stronger blood glucose responses to each of these hormones compared to vehicle
controls; mice treated with 6bK experienced hypoglycemia during insulin tolerance tests (Fig.
3.4b) and hyperglycemia following challenges with either amylin (Fig. 3.4c) or glucagon (Fig.
3.4d) relative to control animals. Similar to glucagon, acute amylin administration in rodents
results in a transient increase in blood glucose levels through gluconeogenesis and activation of
lactic acid flux from muscle tissue to the liver43. Moreover, in each case the plasma level of the
hormone injected remained elevated at the end of the procedure in 6bK-treated mice relative to
control animals, demonstrating a role for IDE in regulating the abundance of these hormones
(Figs. 3.4b to 3.4d insets).
3.8 IDE inhibition promotes glucagon signaling and gluconeogenesis
Taken together, these results strongly suggest that IDE activity regulates the stability and
physiological activities of glucagon and amylin, in addition to insulin. Higher glucagon levels
upon 6bK treatment provide a possible explanation for impaired glucose tolerance observed
during an IPGTT. This model predicts that abrogating glucagon signaling should reverse the
elevation of blood glucose by 6bK treatment during an IPGTT, while not substantially affecting
the signaling pathways through which 6bK treatment lowers blood glucose during an OGTT.
To explicitly test these hypotheses, we repeated the glucose tolerance experiments using
GCGR–/– mice that lack the G-protein coupled glucagon receptor (Fig. 3.5a and 3.5b)44. As
63
expected, mice lacking glucagon signaling exhibited an improvement in oral glucose tolerance
upon 6bK treatment relative to vehicle controls that was similar to the oral glucose tolerance
improvement observed in wild-type mice (Fig. 3.5a), consistent with a model in which insulin
signaling in these mice is intact and regulated by IDE. In contrast, the responses of GCGR–/–
mice treated with 6bK or vehicle alone to i.p. injected glucose were virtually identical, consistent
with a model in which glucagon signaling drives the impaired glucose tolerance of wild-type lean
and DIO mice upon 6bK treatment during an IPGTT (compare Figs. 3.5b and 3.3c).
Collectively, these results reveal that IDE inhibition promotes glucagon signaling that can impair
glucose tolerance during an IPGTT.
64
Figure 3.5 Acute IDE inhibition modulates the endogenous signaling activity of glucagon,
amylin and insulin. a and b, G-protein-coupled glucagon receptor knockout mice (GCGR–/–,
C57BL/6J background) treated with IDE inhibitor 6bK (, 80 mg/kg) display altered glucose
tolerance relative to vehicle-treated mice () if challenged with oral glucose (a) but not i.p.
injected glucose (b). c, Wild-type mice fasted overnight were injected i.p. with pyruvate (2.0
g/kg) 30 min after treatment with 6bK (), inactive analog bisepi-6bK (), or vehicle alone ().
d, Plasma hormone measurements 60 min post-PTT reveal elevated glucagon but similar
insulin levels for the 6bK-treated cohort () relative to bisepi-6bK (), or vehicle () controls.
e, RT-PCR analysis of liver samples 60-min post-PTT revealed elevated gluconeogenesis
transcriptional markers for the 6bK-treated group () relative to vehicle controls (). f, Acute
IDE inhibition slows gastric emptying through amylin signaling. Wild-type mice fasted overnight
were given an oral glucose bolus (3.0 g/kg supplemented with 0.1 mg/mL phenol red) 30 min
after treatment with 6bK alone (), 6bK co-administered with the specific amylin receptor
antagonist AC187 (, 3 mg/kg i.p.), vehicle alone (), or inactive bisepi-6bK (). The
stomachs were dissected at 30 min post-glucose gavage. All data points and error bars
represent mean ± SEM. Significance tests were performed using two-tail Student’s t-test, and
significance levels shown are p < 0.05 (*) or p < 0.01 (**) versus the vehicle-only control group.
0.0
1.0
2.0
3.0
c e f pyruvate tolerance test (PTT)
0
50
100
150
200
250
-60 -30 0 30 60
blo
od
glu
co
se
(m
g/d
L)
minutes post-pyruvate injection (2.0 g/kg)
bisepi (80 mg/kg)
6bK (80 mg/kg)
Vehicle
Rx pyruvate
* * **
6bK
bisepi
(n = 7-8)
a
0
100
200
300
400
-60 -30 0 30 60 90 120
6bK (80 mg/kg)
Vehicle
Rx
oral
glucose
*
**
minutes post-glucose gavage (3.0 g/kg)
(n = 5-6)
b
0
100
200
300
400
-60 -30 0 30 60 90 120
6bK (80 mg/kg)
Vehicle
Rx
i.p.
glucose
(n = 4-6)
minutes post-glucose injection (1.5 g/kg)
oral glucose, GCGR–/– mice injected glucose, GCGR–/– mice
6bK 6bK
blo
od
glu
co
se
(m
g/d
L)
rela
tive
ge
ne
expre
ssio
n
0%
20%
40%
60%
80%
sto
ma
ch
ph
en
ol-
red c
on
ten
t
V 6bK +
AC187
**
amylin-induced gastric
retention of glucose
bis
epi
6bK
liver gluconeogenesis
markers 60 min post-PTT
d
0.00
0.05
0.10
0.15
0.20
0.0
0.2
0.4
0.6
0.8
1.0
glu
ca
go
n (
ng/m
L)
in
su
lin (
ng/m
L)
**
hormone levels
after PTT
V 6bK bis epi
PEPCK G6Pase
* **
V 6bK V 6bK
blo
od
glu
co
se
(m
g/d
L)
65
To investigate the effect of IDE inhibition on endogenously secreted glucagon, we
subjected mice treated with 6bK, vehicle, or inactive bisepi-6bK to a pyruvate tolerance test
(PTT), which measures the ability of the liver under the action of glucagon to use pyruvate as a
gluconeogenic substrate (Fig. 3.5c). The 6bK-treated cohort displayed significantly elevated
plasma glucagon and increased expression of liver gluconeogenic markers compared to both
control groups (Figs. 3.5d and 3.5e). The 6bK cohort also experienced significantly lower blood
glucose during the PTT, suggesting that IDE inhibition produced a concomitant stimulation of
glucose clearance that outweighed its effects on gluconeogenesis (Fig. 3.5c). These results
collectively establish that IDE inhibition can augment endogenous glucagon signaling under
conditions that favor gluconeogenesis.
3.9 IDE inhibition promotes amylin signaling and gastric emptying
Amylin is co-secreted with insulin, and is involved in glycemic control by inhibiting gastric
emptying through the vagal route45, promoting satiety during meals46, and antagonizing
glucagon signaling47. Pramlintide (Smylin) is a synthetic amylin derivative used clinically to
control post-prandial glucose levels33,36,48. To determine the effects of IDE inhibition on
endogenous amylin signaling, we measured gastric emptying efficiency49, an amylin-specific
process, in mice treated with 6bK, inactive control bisepi-6bK, or vehicle alone. Mice treated
with 6bK exhibited 2-fold slower gastric emptying of a labeled glucose solution measured at 30
minutes post-gavage compared to vehicle and bisepi-6bK-treated controls (Fig. 3.5f).
Importantly, co-administration of the specific amylin receptor antagonist AC18750 blocked the
effects of 6bK on gastric emptying (Fig. 3.5f). Collectively, these data reveal that IDE inhibition
can slow post-prandial gastric emptying and demonstrate a role for IDE in modulating amylin
signaling in vivo. These results also suggest that IDE inhibition may mimic the effect of amylin
supplementation with pramlintide during meals2,33.
66
3.10 Implications
The discovery and application of the first potent, highly selective, and physiologically
active small-molecule IDE inhibitor revealed that acute IDE inhibition can lead to improved
glucose tolerance in lean and obese mice after oral glucose administration, conditions that
mimic the intake of a meal. These results validate the potential of IDE as a therapeutic target
following decades of speculation3,4. Our data show that small-molecule IDE inhibitors can
improve oral glucose tolerance to an extent comparable to that of DPP4 inhibitors2,33. The
potential relevance of these animal studies to human disease is supported by the repeated
recognition of IDE as a diabetes susceptibility gene in humans5-11.
Equally important, additional in vivo and biochemical experiments using 6bK led to the
discovery that IDE regulates the stability and signaling of glucagon and amylin, in addition to its
established role in insulin degradation10-12. The identification of two additional pancreatic
hormones as endogenous IDE substrates advances our understanding of the role of IDE in
regulating physiological glucose homeostasis (Fig. 3.6). Amylin-mediated effects on gastric
emptying and satiety during meals have been recently recognized to have therapeutic relevance
in the treatment of diabetes2,33, and our results represent the first demonstration of a small-
molecule that can regulate both amylin and insulin signaling. Moreover, the link between IDE
and glucagon revealed in this study provides additional evidence of the importance of glucagon
regulation in human diabetes51.
67
Figure 3.6 Model for the expanded roles of IDE in glucose homeostasis and gastric
emptying based on the results of this study. IDE inhibition increases the abundance and
signaling of three key pancreatic peptidic hormones, insulin, amylin, and glucagon, with the
corresponding physiological effects shown in blue and red.
Our study also reveals a specific pharmacological requirement for therapeutic IDE
inhibition—namely, that transient, rather than chronic, IDE inhibition is desirable to prevent
elevation of glucagon signaling51 (Fig. 3.6). A potential anti-diabetic therapeutic strategy
motivated by these findings is the development of a fast-acting IDE inhibitor that can be taken
with a meal to transiently augment endogenous insulin and amylin responses to help control
post-prandial glycemia33,34, and that is cleared or degraded before glucagon secretion resumes.
Similar pre-meal therapeutic strategies with short-lived agents have already proven successful
with fast-acting insulin analogs, secretagogues, and amylin supplementation34,35. It is tempting
to speculate these agents may also have synergistic effects when co-administered with an IDE
inhibitor3,52. Alternatively, the combination of an IDE inhibitor with incretin therapy2,33 or a
glucagon
insulin
amylin
6bK
IDE
improved glucose
tolerance
slower gastric empyting
post-prandial gluconeogenesis
H2NNH
O
HN O
HN
O
HN
O
NHO
O
O
NH3+
68
glucagon receptor antagonist51, may also prove therapeutic, as suggested by our experiments
with glucagon-receptor deficient mice. Our findings also raise the possibility that future
generations of IDE modulators may achieve substrate-selective inhibition13 to enable the
selective degradation of substrates such as glucagon while impairing the degradation of insulin.
The identification of a highly selective IDE inhibitor using a DNA-encoded library coupled
with in vitro selection further establishes the value of this approach for the target-based
discovery of bioactive small molecules. The unbiased nature of the selection led to the
identification of a novel small-molecule binding site in IDE that enables unprecedented inhibition
selectivity for this enzyme. These macrocycles and structural insights therefore may also prove
useful in the development of assays that specifically target this binding site, and in the discovery
of novel therapeutic leads that target IDE inhibition. More generally, this work highlights the
value of physiologically active small-molecule probes to characterize the functions of genes
implicated in human disease, an approach that could prove increasingly valuable as human
genomic studies become more prevalent15,16.
3.11 Methods
In vitro selection of a DNA-templated library with immobilized mouse IDE. The in
vitro selection used here was adapted from previously described protocols1,2 using a DNA-
templated library of 13,824 macrocycles3. Recombinant N-His6-tagged mouse IDE42-1019 (isoform
containing the amino acids 42-1019 of the IDE sequence) was purified using immobilized cobalt
magnetic beads (Dynabeads® His-Tag Isolation & Pulldown, Invitrogen®) according to the
manufacturer’s instructions. This purified IDE was confirmed to be catalytically active using the
peptide substrate assay described below. IDE protein (~20 µg) was loaded onto the solid
support by incubating the protein with beads (30 µL) at 25 °C for 30 min in 300 µL of pH 8.0
buffer containing 50 mM phosphate, 300 mM NaCl and 0.01 % Tween-20 (PBST buffer), and
69
washed twice with the same buffer. Two individually prepared protein-bead suspensions were
incubated for 30 min with 5 pmol of the DNA-templated macrocycle library at RT, in pH 7.4
buffer containing 50 mM Tris-HCl, 150 mM NaCl, 0.05 % Tween-20 (TBST buffer)
supplemented with 0.01 % BSA and 3 mg/mL yeast RNA (Ambion®). The beads were washed
three times with 200 µL TBST buffer. The enriched library fraction was eluted by treatment with
200 mM imidazole in PBST buffer (50 µL) for 5 min.
The eluate solution was isolated and purified by buffer exchange using Sephadex spin-
columns (Centrisep, Princeton Separation), according to the manufacturer’s instructions. PCR
amplification of the enriched pool of library barcodes was performed as previously reported1,
using primers that append adaptors for Illumina sequencing and a 7-base identifier. The long
adaptor primer was
5’_AATGATACGGCGACCACCGAGATCTACACTCTTTCCCTACACGACGC
TCTTCCGATCTXXXXXXCCCTGTACAC and the short adaptor primer was 5’_CAAGCAG
AAGACGGCATACGAGCTCTTCCGATCTGAGTGGGATG (the 7-base identifier was XXXXXX).
The PCR amplicons were purified by polyacrylamide gel electrophoresis, extracted, and
quantified using qPCR and Picogreen assays (Invitrogen).
High-throughput DNA sequencing was performed on an Illumina Genome Analyzer
instrument at the Harvard FAS Center for Systems Biology, Cambridge, MA, to yield an average
of ~3.8 million sequence reads for each selection, untreated bead control and pre-selection
library. Deconvolution of library barcodes and enrichment calculations were performed with
custom software as described previously1. Variations in library member abundance as a result
of binding to immobilized IDE was revealed by calculating fold-enrichment over the pre-selection
library for the two independent selection experiments (Extended Data Fig. 1).
70
Protease assays with fluorogenic peptide substrates. The proteases IDE42-1019,
recombinant human IDE42-1019 (R&D Systems), neprilysin (R&D), and angiotensin-converting
enzyme (R&D) were assayed using the fluorophore/quencher-tagged peptide substrate Mca-
RPPGFSAFK(Dnp)-OH (R&D) according to the manufacturer’s instructions and recommended
buffers. For IDE the recommended buffer is 50 mM Tris pH 7.5, 1 M NaCl. The enzyme
mixtures (48 µL) were transferred to a 96-well plate and combined with 2 µL of inhibitor in
DMSO solutions, in 3-fold dilution series. The mixtures were allowed to equilibrate for 10 min
and the enzymatic reaction was started by addition of substrate peptide in assay buffer (50 µL),
mixed, and monitored on a fluorescence plate reader (excitation at 320 nm, emission at 405
nm). Similarly, thimet oligopeptidase (R&D) and neurolysin (R&D) were assayed using
substrate Mca-PLGPK(Dnp)-OH (R&D) according to the manufacturer’s instructions and
recommended buffers. Matrix metalloproteinase-1 (R&D) was activated and assayed according
to the manufacturer’s instructions with substrate Mca-KPLGL-Dpa-AR-NH2 (R&D). All assay
data points were obtained in duplicate. Data for the Yonetani–Theorell double inhibition plot was
generated using 1 µL of each inhibitor (6b, and Ii1 or bacitracin) under otherwise identical
conditions as above, at concentrations corresponding to ⅓x, 1x, 3x and 9x of respective IC50
values against hIDE (R&D).4,5
Protease assays with fluorogenic peptide substrates.IDE degradation assays for
insulin and calcitonin-gene related peptide (CGRP). A solution of 0.4 µg/mL IDE (R&D) in
pH 7.5 buffer containing 50 mM Tris, 1.0 M NaCl (48 µL) was transferred to a 96-well plate, and
combined with 2 µL of each inhibitor (6b, 6bK and 28) dissolved in DMSO, in 3-fold dilution
series (Extended Data Fig. 2c). A solution of insulin (50 µL) was added to a final concentration
of 10 ng/mL, and incubated at 30 °C for 15 min. This procedure was optimized to result in ~75
% degradation of insulin. The reaction was terminated by addition of inhibitor 6bK to a final
71
concentration of 20 µM and chilled on ice. Insulin was quantified using 10 µL of the enzymatic
reaction for the sensitive-range protocol Homogeneous Time-Resolved FRET Insulin assay
(CysBio®) in 20 µL total volume according to the manufacturer’s instructions. Fluorescence
was measured using a Tecan Safire 2 plate reader (excitation = 320 nm, emission = 665 and
620 nm, lag time = 60 µs) according the assay manufacturer’s recommendations. Degradation
of CGRP by endogenous IDE in mouse plasma was analyzed by LC-MS for the formation of
CGRP1-17 and CGRP18-37 as previously reported6. The substrate was added to a final
concentration of 10 µM, and 6b was added to a final concentration of 0.1 to 10 µM (Extended
Data Fig. 2d).
General procedure for synthesis of macrocycle inhibitors. Rink amide resin
(NovaPEG Novabiochem®, ~0.49 mmol/g, typically at a scale of 0.1 to 2 mmol) was swollen
with ~10 volumes of anhydrous DMF for 1 h in a peptide synthesis vessel with mixing provided
by dry nitrogen bubbling. In a separate flask, Nα-allyloxycarbonyl-Nε-2-Fmoc-L-lysine (5 equiv.)
and 2-(1H-7-azabenzotriazol-1-yl)-1,1,3,3-tetramethyl uronium hexafluorophosphate (HATU,
4.75 equiv.) were dissolved in anhydrous DMF (~10 vol.), then treated with N,N'-
diisopropylethylamine (DIPEA, 10 equiv.) for 5 min at RT. The solution was combined with the
pre-swollen Rink amide resin and mixed with nitrogen bubbling overnight. The vessel was
eluted and the resin was washed three times with N-methyl-2-pyrrolidone (NMP, ~10 vol.).
Following each coupling step, Fmoc deprotection was effected with 20 % piperidine in NMP
(~20 vol.) for 20 min, repeated three times, followed by washing three times with NMP (~10 vol.)
and twice with anhydrous DMF (~10 vol.). The general procedure for amide coupling of building
blocks A, B and C was treatment of the resin with solutions of HATU-activated Nα-Fmoc amino
acids (5 equiv.) for 3-5 hours in anhydrous DMF, mixing with dry nitrogen bubbling. The general
72
procedure for HATU-activation was treating a solution of Nα-Fmoc amino acid (5 equiv.) and
HATU (4.75 equiv.) in anhydrous DMF (10 vol.) with DIPEA (10 equiv.) for 5 min at RT.
Following the final Fmoc deprotection procedure, the α-amine of building block C was
coupled with allyl fumarate monoester (10 equiv.) using activation conditions as previously
described with HATU (9.5 equiv.) and DIPEA (20 equiv.) in anhydrous DMF (~10 vol.). Allyl
fumarate coupling was accomplished by overnight mixing with dry nitrogen bubbling, followed by
washing five times with NMP (~10 vol.) and three times with CHCl3 (~10 vol.). Simultaneous
allyl ester and N-allyloxycarbonyl group cleavage in solid support was effected with three
consecutive treatments with a solution of tetrakis(triphenylphosphine)palladium(0) (0.5 equiv.)
dissolved in degassed CHCl3 containing acetic acid and N-methylmorpholine (40:2:1 ratio, ~20
vol.), mixing by nitrogen bubbling for 30 min. The resin was then washed twice subsequently
with ~20 vol. of 5 % DIPEA in DMF, then twice with a 5 % solution of sodium
diethyldithiocarbamate trihydrate in DMF (~20 vol.), twice with 5 % solution of
hydroxybenzotriazole monohydrate in DMF, and finally washed with 50 % CH2Cl2 in DMF and
re-equilibrated with anhydrous DMF (~10 vol.).
Treating the resin with pentafluorophenyl diphenylphosphinate (5 equiv.) and DIPEA (10
equiv.) in anhydrous DMF (~10 vol.) mixing by nitrogen bubbling overnight produced the
macrocyclized products. The resin was washed with NMP (~20 vol.) and CH2Cl2 (~20 vol.) and
dried by vacuum. The macrocyclized product was cleaved from the resin by two 15 min
treatments of the macrocycle-bound resin with 95 % TFA containing 2.5 % water and 2.5 %
triisopropylsilane (~20 vol.), followed by two TFA washes (~5 vol.). The TFA solution was dried
to a residue under rotatory evaporation, and the peptide was precipitated by the addition of dry
Et2O. The ether was decanted and the remaining solid was dried and dissolved in a minimum
volume of 3:1 DMF-water prior to purification by liquid chromatography. HPLC purification was
performed on a C18 21.2x250 mm column (5 µm particle, 100 Å pore size, Kromasil®), using a
gradient of 30 % to 80 % MeCN/water over 30 min, and solvents containing 0.1 % TFA.
73
Fractions containing the desired macrocyclic peptide were combined and freeze-dried to
produce a white powder. Typical yields were 5-15 % based on resin loading. Purity was
determined by HPLC (Zorbax SB-C18 2.1x150 mm column, 5 µm particle) with UV detection at
230 nm, using a gradient of 30 % to 80 % MeCN/water over 30 min, and solvents containing 0.1
% TFA. The formula of final products was confirmed by accurate mass measurements using an
Agilent 1100 LC-MSD SL instrument (Supplementary Table S2).
Dosing and formulation of macrocycle inhibitors for in vivo studies. The doses of 6bK
used in this study were chosen based on literature precedent for small molecules and drugs of
similar potencies7-13. Procedures using experimental compounds were in accordance with the
standing committee on the Use of Animals in Research and Teaching at Harvard University, the
guidelines and rules established by the Faculty of Arts and Sciences' Institutional Animal Care
and Use Committee (IACUC), and the National Institutes of Health Guidelines for the Humane
Treatment of Laboratory Animals.
Purified macrocycle inhibitors were dissolved in DMSO-d6 (~200 to 250 mg/mL stock
solutions). A sample aliquot (5 µL) of the macrocycle solution was diluted with 445 µL DMSO-
d6, then combined with 50 µL of freshly prepared solution of 20 mM CH2Cl2 in DMSO-d6 in for
1H-NMR acquisition (600 MHz, relaxation time = 2 sec). The inhibitor concentration was
calculated using the integral of the CH2Cl2 singlet (δ 5.76 ppm, 2H)14, which appears in an
uncluttered region of these spectra1,15. For injectable formulations (10 mL/kg i.p. injection
volume), the macrocycle inhibitor solution in DMSO-d6 (200 – 250 mg/mL, based on free-base
molecular weight) was combined with 1:20 w/w Captisol® powder (CyDex)16. The resulting
slurry was supplemented with DMSO-d6 to make up to 5 % of the final formulation volume,
mixed thoroughly and dissolved with sterile saline solution (0.9 % NaCl). Vehicle controls were
identically formulated with 5 % DMSO-d6 and equal amount of Captisol®. The formulated
74
solutions of inhibitor were clear with no visible particles, and were stored overnight at 4 °C prior
to injection.
Expression and purification of recombinant cysteine-free hIDE (IDE-CF). We
expressed cysteine-free catalytically-inactive, human IDE (IDE-CF) in pPROEX vector17. IDE-
CF contains the following substitutions: C110L, E111Q, C171S, C178A, C257V, C414L, C573N,
C590S, C789S, C812A, C819A, C904S, C966N, and C974A. IDE was expressed and purified
as previously described17. Briefly, IDE-CF was transformed into E. coli BL21-CodonPlus (DE3)-
RIL, grown at 37 °C to a cell density of 0.6 O.D. and induced with IPTG at 16 °C for 19 hours.
Cells were lysed and the lysate was subjected to Ni-affinity (GE LifeScience) and anion
exchange chromatography (GE LifeScience). The protein was further purified by size exclusion
chromatography (Superdex S200 column) three successive times, first without inhibitor then two
times after addition of 2-fold molar excess of 6b.
IDE-CF•6b co-crystallization. Eluent from size exclusion chromatography was
concentrated to 20 mg/ml in 20 mM Tris, pH 8.0, 50 mM NaCl, 0.1 mM PMSF and 2-fold molar
excess of 6b was added to form the protein-inhibitor complex. The complex was mixed with
equal volumes of reservoir solution containing 0.1 M HEPES (pH 7.5), 20 % (w/v) PEGMME-
5000, 12 % tacsimate and 10 % dioxane. Crystals appeared after 3-5 days at 25 °C and were
then equilibrated in cryoprotective buffer containing well solution and 30 % glycerol. IDE-CF•6b
complex crystals belong to the space group P65, with unit-cell dimensions a = b = 262 Å and c =
90 Å, and contain two molecules of IDE per asymmetric unit (Extended Data Figure 3a).
75
X-Ray Diffraction. X-ray diffraction data were collected at the National Synchrotron
Light Source at Brookhaven National Laboratories beamline X29 at 100K and 1.075 Å.
IDE-CF•6b structure determination. Data were processed in space group P65 using
autoProc18. The structure was phased by molecular replacement using the structure for human
IDE E111Q (residues 45-1011, with residues 965-977 missing) in complex with inhibitor
compound 41367 (PDB: 2YPU) as a search model in Phaser19. The model of the structure was
built in Coot20 and refined in PHENIX21, using NCS (torsion-angle) and TLS (9 groups per
chain). In the Ramachandran plot, 100 % of the residues appear in the allowed regions, 97.2 %
of the residues appear in the favored regions, and 0 % of the residues appear in the outlier
regions (Extended Data Figure 3a). The structural model of IDE and inhibitor was refined using
non-crystallographic symmetry restraints due to the high degree of structural similarity between
the two chains of the protein the asymmetric unit. The root-mean-square deviation between the
two chains is 0.5 Å for the protein chains, and 0.9 Å for the ligand atoms, indicating high
structural similarity between the two chains. Structure coordinates are deposited in the Protein
Data Bank (accession number 4TLE).
Macrocycle docking simulations. Receptor and ligand preparation was performed in
the standard method22,23. DOCKing was performed using version 6.6 with default parameters
for flexible ligand and grid-based scoring, and the van der Waals exponent was 9. Because of
the mutagenesis data strongly pointing to a role of Ala479, we limited docking of the macrocycle
to an area within 15 Å of Ala479. The highest scoring poses (Extended Data Fig. 3), by both
gridscore5 and Hawkins GB/SA6, are consistent with the placement of building blocks A
(benzophenone), B (cyclohexyl ring), and trans olefin of 6b in the proposed structure. Docking
calculations for the inactive isomer 6a were unsuccessful, while for the low-activity analog 11
76
the result was a different and lower-scoring pose than 6b, consistent with the mutagenesis and
biochemical assay results (Table S5, Fig. 1b, Extended Data Fig. 4).
Anisotropy binding assay. Catalytically-inactive CF-IDE was titrated with fluorescein-
labeled macrocycle 31 in 20 mM Tris buffer pH 8.0, with 50 mM NaCl, and 0.1 mM PMSF at
25°C in the presence or absence of insulin (2.15 µM). The final assay volume was 220 µL, with
a final DMSO concentration of 0.1 % and a final 31 concentration of 0.9 nM. After equilibration,
the increase in the fluorescence anisotropy of the fluorescent ligand was recorded at 492 nm,
using excitation at 523 nm, and fitted against a quadratic binding equation in Kaleidagraph
(Synergy Software) to yield the dissociation constant (KD = 43 nM). From our structural work,
we hypothesized that insulin and macrocycle 31 compete for the same binding site.
Equation 124 approximates how the concentration of insulin ([I]) and the affinity constant
of insulin (Ki = 280 nM) affect the apparent dissociation constant (KDapp) of macrocycle 31 for
CF-IDE. In the absence of competing insulin, 31 binds with the dissociation constant (KD = 43
nM) to CF-IDE. In the presence of 2.15 uM insulin, the calculated KDapp for macrocycle 31 is
363 nM (~8-fold shift) which is in good agreement with the competitive binding mode revealed
by the crystal structure, and the anisotropy measurements (observed ~7-fold shift, KDapp= ~ 280
nM, Extended Data Fig. 3e).
Eq. 1
Site-directed mutagenesis, expression, and purification of human IDE. The
reported N-His6-tagged human IDE42-1019 construct was introduced in the expression plasmid
pTrcHis-A (Invitrogen) using primers for uracil-specific excision reactions (USER) by Taq (NEB)
and Pfu polymerases (PfuTurbo CX®, Agilent). The IDE gene was amplified with the primers 5’-
KDapp = 1 +
[ I ]
Ki
. KD
77
ATCATCATATGAATAATCCAGCCA-dU-CAAGAGAATAGG and 5’-
ATGCTAGCCATACCTCAGA G-dU-TTTGCAGCCATGAAG (underlined sequences represent
overhangs, and italics highlight the PCR priming sequence). Similarly, the pTrcHis-A vector
was amplified for USER cloning with the primers 5’-ATGGCTGGATTATTCATATGATGA-dU-
GATGATGATGAGAACCC and 5’-ACTCTGAGGTATGGCTAGCA-dU-GACTGGTG. Mutant
IDE constructs were generated by amplifying the full vector construct with USER cloning
primers introducing a mutant overhang (Supplementary Table S3).
All PCR products were purified on microcentrifuge membrane columns (MinElute®,
Quiagen) and quantified by UV absorbance (NanoDrop). Each fragment (0.2 pmol) was
combined in a 10 µL reaction mixture containing 20 units DpnI (NEB), 0.75 units of USER mix
(Endonuclease VIII and Uracil-DNA Glycosylase, NEB), 20 mM Tris-acetate, 50 mM potassium
acetate, 10 mM magnesium acetate, 1 mM dithiothreitol at pH 7.9 (1x NEBuffer 4). The
reactions were incubated at 37 °C for 45 min, followed by heating to 80 °C and slow cooling to
30 °C (0.2 °C/s). The hybridized constructs were directly used for heat-shock transformation of
chemically competent NEB turbo E. coli cells according to the manufacturer’s instructions.
Transformants were selected on carbenicillin LB agar, and isolated colonies were cultured
overnight in 2 mL LB.
The plasmid was extracted using a microcentrifuge membrane column kit (Miniprep®,
Qiagen), and the sequence of genes and vector junctions were confirmed by Sanger
sequencing (Supplementary Table S4). The plasmid constructs were transformed by heat-
shock into chemically-competent expression strain Rosetta 2 (DE3) pLysS E. coli cells (EMD
Millipore), and selected on carbenicillin/chloramphenicol LB agar. Cells transformed with IDE
pTrcHis A constructs were cultured overnight at 37 °C in 2 XYT media (31 g in 1L) containing
100 μg/mL ampicillin and 34 μg/mL chloramphenicol. Expression of His6-tagged IDE proteins
was induced when the culture measured OD600 ~0.6 by addition of isopropyl-β-D-1-
78
thiogalactopyranoside (IPTG) to 1 mM final concentration, incubated overnight at 37 °C,
followed by centrifugation at 10,000 g for 30 min at 4 °C.
Recombinant His6-tagged proteins were purified by Ni(II)-affinity chromatography (IMAC
sepharose beads, GE Healthcare®) according to the manufacturer’s instructions. The cell
pellets were resuspended in pH 8.0 buffer containing 50 mM phosphate, 300 mM NaCl, 10 mM
imidazole, 1 % Triton X-100 and 1 mM tris(2-carboxyethyl)phosphine hydrochloride (TCEP), and
were lysed by probe sonication for 4 min at <4 °C, followed by clearing of cell debris by
centrifugation at 10,000 g for 25 min at 4 °C. The supernatant was incubated with Ni(II)-doped
IMAC resin (2 mL) for 3 h at 4 °C. The resin was washed twice with the cell resuspension/lysis
buffer, and three times with pH 8.0 buffer containing 50 mM phosphate, 300 mM NaCl, 50 mM
imidazole and 1 mM TCEP. Elution was performed in 2 mL aliquots by raising the imidazole
concentration to 250 mM and subsequently to 500 mM in the previous buffer. The fractions
were combined and the buffer was exchanged to the recommended IDE buffer (R&D) using spin
columns with 100 KDa molecular weight cut off membranes (Millipore). Protein yields were
typically ~10 µg/L, and >90 % purity based on gel electrophoresis analysis (Coomassie stained).
IDE-specific protease activity was >95 % as assessed by inhibition of degradation of peptide
substrate Mca-RPPGFSAFK(Dnp)-OH (R&D) by 20 µM 6bK, compared with pre-quantitated
commercially available human IDE (R&D). The complete list of IDE mutations assayed is shown
in Supplementary Table S5.
In vivo studies, general information. Wild-type C57BL/6J and diet-induced obese
(DIO) C57BL/6J age-matched male adult mice were purchased from Jackson Laboratories. The
age range was 13 to 15 weeks for lean mice, and 24 to 26 weeks for DIO mice. All animals
were individually housed on a 14-h light, 10-h dark schedule at the Biology Research
Infrastructure (BRI), Harvard University. Cage enrichment included cotton bedding and a red
plastic hut. Water and food were available ad libitum, consisting respectively of normal chow
79
(Prolab® RHM 3000) or high-fat diet (60 kcal % fat, D12492, Research Diets Inc.). Adult IDE
knock-out mice (IDE–/–) and control mice (IDE+/+) were obtained from Mayo Clinic (Florida), and
housed in the Biology Research Infrastructure (BRI), Harvard University, for 8 weeks prior to
experiments as described above. Experiments were conducted on IDE–/– and +/+ age-matched
mice cohorts ranging 17 to 21 weeks old. All animal care and experimental procedures were in
accordance with the standing committee on the Use of Animals in Research and Teaching at
Harvard University, the guidelines and rules established by the Faculty of Arts and Sciences'
Institutional Animal Care and Use Committee (IACUC), and the National Institutes of Health
Guidelines for the Humane Treatment of Laboratory Animals. Glucagon-receptor knock-out
mice (GCGR–/–) and control WT mice (GCGR+/+) were group-housed with a 14-h light and 10-h
dark schedule and treated in accordance with the guidelines and rules approved by the IACUC
at Albert Einstein College of Medicine, NY. Power analysis to determine animal cohort numbers
was based on preliminary results and literature precedent, usually requiring between 5 and 8
animals per group. Animals were only excluded from the cohorts in cases of chronic weakness,
which occurs among GCGR–/– mice, or when we identified occasional DIO mice with an outlier
diabetic phenotype (e.g. >200 mg/dL fasting blood glucose). Age- and weight-matched mice
were randomized to each treatment group. Double-blinding was not feasible.
Glucose tolerance tests GTT and blood glucose measurements. Prior to a glucose
challenge, the animals were fasted for 14 h (8 pm to 10 am, during the dark cycle) while
individually housed in a clean cage with inedible wood-chip as a floor substrate, cotton bedding
and a red plastic hut. Inhibitor, vehicle or control compounds were administered by a single
intraperitoneal (i.p.) injection 30 min prior to the glucose challenge. Dextrose was formulated in
sterile saline (3 g in 10 mL total), and the dose was adjusted by fasted body weight. For oGTT,
3.0 g/kg dextrose was administered by gavage at a dose of 10 mL/kg, and for ipGTT, 1.5 g/kg
80
dextrose injected at a dose of 5 mL/kg. Blood glucose was measured using AccuCheck®
meters (Aviva) from blood droplets obtained from a small nick at the tip of the tail, at timepoints -
45, 0, 15, 30, 45, 60, 90 and 120 min with reference to the time of glucose injection. The area
of the blood glucose response profile curve corresponding to each animal was calculated by the
trapezoid method25, using as reference each individual baseline blood glucose measurement
prior to glucose administration (t = 0). The sum of the trapezoidal areas between the 0, 15, 30,
45, 60, 90 and 120 minute time points corresponding to each animal were summed to obtain the
area under the curve (AUC). The relative area values are expressed as a percentage relative to
the average AUC of the vehicle cohort, which is defined as 100 % (Extended Data Fig 9).
Values are reported as mean ± S.E.M. Statistics were performed using a two-tail Student’s t-
test, and significance levels shown in the figures are * p < 0.05 versus vehicle control group or
** p < 0.01 versus vehicle control group.
Insulin Tolerance Test (ITT), Glucagon Challenge (GC) and Amylin Challenge (AC)
For hormone challenges animals were fasted individually housed as described above. For ITT
the fasting period was 6 h (7 am to 1 pm), and for glucagon and amylin challenges the fasting
period was 14 h (8 pm – 10 am). Inhibitor or vehicle alone was injected i.p. as previously
described, 30 min prior to each hormone challenge. Insulin (Humulin-R®, Eli Lilly) was injected
subcutaneously (s.c.) 0.25 U/kg formulated in sterile saline (5 mL/kg). Glucagon (Eli Lilly) was
injected s.c. 100 µg/kg formulated in 0.5 % BSA sterile saline (5 mL/kg). Amylin (Bachem) was
injected s.c. 250 µg/kg formulated in sterile saline (5 mL/kg). Blood glucose was measured at
timepoints -45, 0, 15, 30, 45, 60 and 75 min with reference to the time of hormone injection, by
microsampling from a tail nick as described above. Values are reported as mean ± S.E.M.
Statistics were performed using a two-tail Student’s t-test, and significance levels shown in the
figures are * p < 0.05 versus vehicle control group or ** p < 0.01 versus vehicle control group.
81
Blood collection and plasma hormone measurements. Blood was collected in
EDTA-coated tubes (BD Microtainer®) from trunk bleeding (~500 µL) after CO2-euthanasia for
all hormone assays. The plasma was immediately separated from red blood cells by
centrifugation 10 min at 1800 g, aliquoted, frozen over dry ice and stored at -80 °C. Insulin,
glucagon, amylin and pro-insulin C-peptide fragment were quantified from 10 µL plasma
samples using magnetic-bead Multiplexed Mouse Metabolic Hormone panel (Milliplex, EMD
Millipore) according to the manufacturer’s instructions, using a Luminex FlexMap 3D instrument.
Plasma containing high levels of human insulin (Humulin-R) were quantified using 25 µL
samples with Insulin Ultrasensitive ELISA (ALPCO). Values are reported as mean ± S.E.M.
Statistics were performed using a two-tail Student’s t-test, and significance levels shown in the
figures are * p < 0.05 versus vehicle control group or ** p < 0.01 versus vehicle control group.
Gastric emptying measurements. Mice were fasted 14 h (8 pm to 10 am). Inhibitor or
vehicle alone was injected i.p. as previously described, followed 30 min later by an oral glucose
bolus (3.0 g/kg, 10 mL/kg) in sterile saline containing 0.1 mg/mL phenol red. At 30 min, the
stomach was promptly dissected after CO2-euthanasia and stored on ice. The stomach
contents were extracted into 2.5 mL EtOH (95 %) by homogenization for 1 min using a probe
sonicator. Tissue debris were decanted by centrifugation at 4000 g, followed by clearing at
15000 g for 15 min. The supernatant (1 mL) was mixed with 0.5 mL of aqueous NaOH (20
mM), and incubated at -20 °C for 1 h. The solution was centrifuged at 15,000 g for 15 min, and
absorbance was determined at 565 nM. The spectrophotometer was blanked with the stomach
contents of a mouse treated with colorless glucose solution. The absorbance was adjusted to
the amount of glucose solution dosed to each mouse. Values are reported as mean ± S.E.M
relative to the original phenol red glucose solution. Statistics were performed using a two-tail
82
Student’s t-test, and significance levels shown in the figures are * p < 0.05 versus vehicle
control group or ** p < 0.01 versus vehicle control group.
Stable isotope dilution LC-MS, pharmacokinetics, and tissue distribution
measurements. Heavy-labeled macrocycle inhibitor (heavy-6bK, Extended Data Fig. 5) was
synthesized as described above, substituting “building block C” with Nα-Fmoc-Nε-Boc-lysine 13C6
15N2 (98 atom %, Sigma-Aldrich). The product was 8 mass-units heavier than 6bK, otherwise
with identical properties and IC50. Plasma samples (15 µL) from 6bK-treated mice and vehicle
controls were combined with 5 µL of heavy-6bK in PBS (final concentration of 10 µM), and
incubated for 30 min on ice. Plasma proteins were precipitated with 180 µL cold 1 % TFA in
MeCN, sonicated 2 min, and centrifuged 13,000 g for 1 min. The supernatant was diluted 100-
and 1000-fold for liquid chromatography-mass spectrometry (LC-MS) analysis. Tissue samples
(~100 mg) from 6bK-treated mice and vehicle controls were weighed and disrupted in Dounce
homogenizers with PBS buffer (0.5 mL/100 mg sample), supplemented with 5 µM heavy-6bK
and protease inhibitor cocktail (1 tablet/50 mL PBS, Roche diagnostics). The lysate was
incubated on ice for 30 min, sonicated 5 min and centrifuged at 13,000 g for 5 min. The bulk of
supernatant proteins were precipitated by denaturation at 95 °C for 5 min, removed by
centrifugation. A 50 µL aliquot of the supernatant was treated with 450 µL cold 1 % TFA in
MeCN, cleared by centrifugation and diluted 100-fold for LC-MS analysis as described above for
plasma samples. A standard curve of 6bK and heavy-6bK (1 µM each and 3-fold serial
dilutions) were used for LC-MS quantitation using a Waters Q-TOF premier instrument.
RT-PCR analysis of liver gluconeogenesis markers phosphoenolpyruvate
carboxykinase (PEPCK) and glucose-6-phosphatase (G6Pase). Total RNA was isolated
from liver samples (~100 mg) using TRIzol® reagent (Invitrogen, 1 mL/100 mg sample),
followed by spin-column purification (RNeasy® kit, Qiagen) and on-column DNAse treatment
83
(Qiagen) according to the manufacturer’s instructions. RNA concentrations were determined by
UV spectrophotometry (NanoDrop). One microgram of total RNA was used for reverse
transcription with oligo(dT) primers (SuperScript® III First-Strand Synthesis SuperMix, Life
Technologies) according to the manufacturer’s instructions. Quantitative PCR reactions
included 1 µL of cDNA diluted 1:100, 0.4 µM primers, 2x SYBR Green PCR Master Mix
(Invitrogen) in 25 µL total volume, and were read out by a CFX96™ Real-Time PCR Detection
System (BioRad). Transcript levels were determined using two known primer pairs26,27 for each
gene of interest (Supplementary Table S4), which were normalized against tubulin and beta-
actin transcripts (ΔΔCT method), and expressed relative to the lowest sample. Duplicate control
assays without reverse transcriptase treatment were run for each RNA preparation and primer
set used. Statistics were performed using a two-tail Student’s t-test, and significance levels
shown in the figures are * p < 0.05 versus vehicle control group or ** p < 0.01 versus vehicle
control group.
Amyloid peptide measurements. Lean C57BL/6J mice were treated with 6bK (80
mg/kg), vehicle alone, or bisepi-6bK (80 mg/kg). Two hours post-injection, hemibrains were
promptly dissected after CO2-euthanasia and stored at -80 °C until extraction. A hemibrain
(~150 mg wet weight) was homogenized in a Dounce homogenizer in 0.2% diethylamine and 50
mM NaCl (900 µL). The homogenate was centrifuged at 20,000 × g for 1 h at 4°C to remove
insoluble material. A fraction of supernatant (100 µL) was neutralized with 1:10 volume of Tris
HCl, pH 6.8. The sample was diluted 1:4 in assay buffer, and analyzed for Aβ(40) and Aβ(42)
levels using the respective Aβ ELISA assays (Invitrogen) following the manufacturer’s protocols.
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Appendix 1
Metabolomics Experiments to identify E.Coli derived ligand of MR1
This Appendix is adapted from:
Jacinto, L et al. MAIT Recognition of a Stimulatory Bacterial Antigen Bound to MR1. The Journal
of Immunology. 2013
91
A1.1 Introduction
MR1-restricted Mucosal Associated Invariant T (MAIT) cells represent a sub-population
of αβ T cells with innate-like properties and limited TCR diversity. MAIT cells are of interest due
to their reactivity against bacterial and yeast species, suggesting they play a role in defense
against pathogenic microbes. Despite the advances in understanding MAIT cell biology, the
molecular and structural basis behind their ability to detect MR1-antigen complexes is unclear.
Here we present our structural and biochemical characterization of MAIT TCR engagement of
MR1 presenting an E. coli-derived stimulatory ligand, rRL-6-CH2OH previously found in
Salmonella typhimurium. We show a clear enhancement of MAIT TCR binding to MR1 due to
presentation of this ligand. Our structure of a MAIT TCR/MR1/rRL-6-CH2OH complex shows an
evolutionarily conserved binding orientation, with a clear role for both the CDR3α and CDR3β
loops in recognition of the rRL-6-CH2OH stimulatory ligand. We also present two additional
xeno-reactive MAIT TCR/MR1 complexes that recapitulate the docking orientation documented
previously despite having variation in the CDR2β and CDR3β loop sequences. Our data
supports a model by which MAIT TCRs engage MR1 in a conserved fashion, their binding
affinities modulated by the nature of the MR1 presented antigen or diversity introduced by
alternate Vβ usage or CDR3β sequences.
A1.2 Results
These results prompted us to analyze by mass spectrometry the content of the hbMR1
in both E. coli exposed and non-exposed protein samples. Normal Phase QTOF analysis clearly
identified a compound with a retention time of ~ 7 minutes present only in the E. coli treated
sample (Figure 2A). Mass spectrometry analysis of this compound determined a compound with
a m/z ratio of 329.1095 and whose fragmentation yielded a pattern nearly identical to that found
for rRL-6-CH2OH (r-RL) (Figure 2B), a MAIT cell stimulatory ligand characterized from
Salmonella typhimurium supernatant10. This compound is generated as a by-product of the
92
riboflavin synthesis pathway and its structure comprises a lumazine core and a ribityl chain
(Figure 2A, inset). rRL-6-CH2OH has been shown to trigger MAIT cell activation in a MR1
dependent manner, and displayed the strongest potency in activating MAIT cells among three
structurally related compounds10. Thus, the increased MAIT TCR affinity to the E. coli-treated
hbMR1 sample correlates with the presence of this ribityl moiety, which our model suggested9
directly participates in MAIT TCR recognition of MR1 presented antigen.
93
Figure A1.1 MAIT Recognition of a Stimulatory Bacterial Antigen Bound to MR1. MS
reveals the presence of rRL-6-CH2OH in the E. coli–treated hbMR1 sample. (A) Extracted ion
chromatograms (EICs) for rRL-6-CH2-OH (m/z 329.1103) from hbMR1 protein exposed to E. coli
(lower panel) compared with untreated protein control (upper panel). EIC shows compound with
m/z 329.1103 present only in E. coli–treated sample (inset). (B) Compound with m/z 329.1095
(left peak, upper panel) from the E. coli–treated hbMR1 sample and product ions from targeted
fragmentation (lower panel); the structures of each of the products of the fragmentation are
shown as insets. The precursor ion is indicated by a diamond. Tandem mass spectrometry
(MS/MS) product ion data match against the theoretical fragmentation pattern of rRL-6-CH2OH
(right peak, upper panel) within <5 ppm.
94
A1.3 Methods
Mass spectrometry analysis of hbMR1. 6.25 µg of DMRL (m/z 325.1154) was injected
onto a Luna NH2 4.6x50 mm, 5 µm column. The flow was analyzed by ESI-TOF-MS on a
Bruker maXis impact QTOF with Agilent 1290 HPLC using a binary gradient of 95% B to 0%
over 5 minutes (A: 20 mM ammonium acetate in water, pH 9.0; B: Acetonitrile). Target ion
detected after elution with aqueous gradient; data was collected in negative ion mode. Retention
time was obtained by extracted ion chromatogram of respective m/z; product ions were obtained
by tandem MS with a collision energy of 20eV. For hbMR1, comparison of hbMR1 protein that
was exposed to E. coli sn and an untreated control hbMR1 sample were analyzed on a Bruker
maXis impact QTOF LC/MS in negative ion mode. 5 uL each of 25 µM hbMR1 was injected onto
a Luna NH2 4.6x50 mm, 5 um column in 20 mM ammonium acetate, pH 9 buffer and eluted with
an aqueous gradient as described above. Retention time of rRL-6-CH2OH was determined by
extracted ion chromatograms using the m/z values. Product ions were obtained from target
fragmentation at collision induced voltages of 20.
95
Appendix 2 Evaluation of Potent α/β -Peptide Analogue of GLP-1 with
Prolonged Action In Vivo
Adapted from prepared manuscript:
Johnson, LM et al. Proteolysis in the Context of Diabetes: Evaluation of Potent α/β-Peptide
Analogue of GLP-1 with Prolonged Action In Vivo. 2014
96
A2.1 Introduction
Glucagon-like peptide-1 (GLP-1) is the natural agonist for GLP-1R, a G protein-coupled
receptor (GPCR) that is displayed on the surface of pancreatic β cells. Activation of GLP-1R
augments glucose-dependent insulin release from β cells and promotes β cell survival. These
properties are attractive for treatment of type 2 diabetes, but GLP-1 is rapidly degraded by
peptidases in vivo. Efforts to develop small-molecule agonists of GLP-1R have not been
successful, presumably because receptor activation requires contact over an extended surface.
All potent GLP-1R agonists reported to date are comprised exclusively of α-amino acid
residues, with prolonged in vivo activity achieved by variations in sequence, incorporation of
stabilizing appendages, and/or specialized delivery strategies. We describe an alternative
design strategy for retaining GLP-1-like function but engendering prolonged activity in vivo,
based on strategic replacement of native α residues with conformationally constrained β-amino
acid residues. This approach may be generally useful for developing stabilized analogues of
peptide hormones. As part of this collaboration, with the Gellman laboratory at University of
Wisconsin, Madison, I ran comparative glucose tolerance tests in mice to assay the efficacy of
different GLP-1 analogues.
A2.2 Results
The ability of α/β -peptide 6 to augment insulin secretion from mouse pancreatic islets in
response to elevated glucose led us to evaluate the activity of this GLP-1 analogue in vivo via
glucose tolerance tests (GTT) (Figure 3). In addition to the α/β -peptide and GLP-1(7-37)-NH2,
these studies included exendin-4 (39 residues), all three of which were tested for the ability to
normalize circulating glucose levels. GLP-1, exendin-4 and α/β -peptide 6 were compared at a
dose of 1 mg/kg, and descending doses were examined for the α/β -peptide. For mice injected
with vehicle rather than peptide (negative control), the intraperitoneal glucose challenge causes
a rapid rise in blood glucose concentration that subsides after 30 min (Figure 3A-B). Mice
97
injected with GLP-1, exendin-4 or α/β -peptide 6 at 1 mg/kg showed a dramatic suppression in
the rise of glucose relative to vehicle-treated mice during the GTT; the three compounds were
equally effective at this dose. Dose-response behavior was observed for 6, with glucose control
maintained at 0.1 mg/kg, but not at 0.01 mg/kg.
In order to determine whether the GLP-1R agonists display prolonged action, I repeated
the GTT 5 hr after agonist administration (Figure 3C). Mice treated with GLP-1(7-37)-NH2
showed no significant difference from those treated with vehicle 30 min after the second glucose
challenge; this result is expected based on the rapid enzymatic inactivation of GLP-1 in vivo. In
contrast, the glucose-lowering effect of exendin-4 is maintained at 5 hr, which is consistent with
prior observations. Exendin-4 persists longer in the bloodstream than does GLP-1 because
exendin-4 is not cleaved by DPP-4 and is only very slowly degraded by neprilysin or other
peptidases.12,13 α/β -Peptide 6 exerted the same glucose-lowering effect at 5 hr as exendin-4
(each at 1 mg/kg). The ability of 6 to induce control of blood glucose levels at 5 hr was
manifested even when the α/β -peptide was administered at 0.1 mg/ml. These results
presumably reflect the resistance of this α/β -peptide to degradation by either DPP-4 or
neprilysin.
98
Figure A2.1 α/β-peptide 6 demonstrates long lasting improvement of in vivo glucose
tolerance.
A) Plasma glucose values during a glucose tolerance test (GTT) for mice treated with GLP-1(7-
37)-NH2 (1 mg/kg), Exendin-4 (Ex-4, 1 mg/kg), varying doses (0.01-1 mg/kg) of α/β-peptide 6 or
vehicle. Upward arrow indicates timing of the peptide treatments delivered via IP injection.
Results show mean (± SEM) of 4 separate mice per condition. B) Average area under the curve
(AUC) values for the GTT data shown in A. C) Plasma glucose values at 30 mins following a
second GTT that was conducted 5 hr following that shown in A. *, P < 0.05 vs. vehicle.
99
A2.3 Discussion
Our results show that a GLP-1- -
amino acid residues with conformationally constrained β-amino acid residues can maintain
native-like agonist activity at the GLP-1 receptor. α/β -Peptide 6 mimics GLP-1 in terms of
augmenting glucose-stimulated insulin secretion from pancreatic β cells and regulating blood
glucose levels in vivo. The prolonged effect of this α/β -peptide relative to GLP-1 is attributed to
the strongly diminished susceptibility to degradation by widely distributed peptidases, a property
that arises in part from the multiple β residue replacements. The favorable characteristics
displayed by α/β -peptide 6 in vitro and in vivo suggest that backbone-modification strategies
involving periodic replacement of α residues with β residues may prove to be generally useful
for developing potent and highly stable analogues of peptide hormones and other signaling
peptides for which the receptor-bound conformation is at least partially α-helical. Side chain
cross-links have been widely employed for this purpose in the past,17-29 but recent structural
studies have revealed that the large additional molecular surfaces generated by the cross-link
itself can make intimate contacts with partner protein surfaces.44-46 Such contacts might alter
binding affinity and/or selectivity relative to the natural prototype. Periodic α-to-β replacement
may represent a more effective approach to retaining an α-helix-like shape47 and the binding
selectivity of a prototype α-peptide while diminishing susceptibility to proteolytic action.
A2.4 Method
Glucose Tolerance Test (GTT). GLP-1(7-37)-NH2, exendin-4 or α/β-peptide 6 was
administered to mice by interperitoneal (i.p.) injection at a 1 mg/kg dose, or lower for α/β-peptide
6, using an injection volume of 10 mL/kg body mass. Each peptide was first dissolved in
prefiltered DMSO at 10 mg/mL concentration, then diluted >20-fold with TBS buffer, pH 7.4
(final DMSO conc. = <5%). Glucose was administered by i.p. injection with a sterile-filtered 30%
D-glucose-saline solution at a 1.5 g/kg dose using a 5 mL/kg injection volume.
100
Thirteen-week-old male C57BL/6J mice (n = 4) were fasted overnight on wood chip
bedding for 15 hours prior to the experiment. Blood glucose levels were monitored from a tail tip
bleed using an ACCU-CHEK Aviva blood glucose meter. Fasting glucose levels were
measured at 75 minutes prior to the glucose injection (t = -75 min), and the compound injection
was performed 60 minutes prior to the glucose injection (t = -60 min). Glucose levels were
measured immediately prior to the glucose injection (t = 0 min) to assess any changes in the
baseline glucose caused by peptide administration. Blood glucose levels were monitored at 30,
60, 90, and 120 minutes after injection of glucose.
Five hours after peptide injection, the mice received a second injection of 1.5 g/kg
glucose. Blood glucose was monitored at 30 min after this second glucose injection. Mice were
sacrificed by CO2 inhalation at the conclusion of the GTT.
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Verdine, G.L. & Korsmeyer, S.J. Activation of apoptosis in vivo by a hydrocarbon-stapled BH3
helix. Science 305, 1466-70, (2004).
102
-helix constrained by
main-chain hydrogen-bond surrogate. J. Am. Chem. Soc. 126, 12252-3, (2004).
26. Verdine, G.L. & Hilinski, G.J. Stapled peptides for intracellular drug targets. Meth. Enzymol.
503, 3-33, (2012).
27. Okamoto, T., Zobel, K., Fedorova, A., Quan, C., Yang, H., Fairbrother, W.J., Huang, D.C.
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(BimSAHB) does not necessarily enhance affinity of biological activity. ACS Chem. Biol. 8, 297-
302, (2013).
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S., Guido, M., Stanislaus, S., Ma, M., Li, H., Rose, M.J., Poppe, L., & Veniant, M.M. Design and
synthesis of conformationally constrained glucagon-like peptide-1 derivatives with increased
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29. Murage, E.N., Gao, G.Z., Bisello, A., & Ahn, J.M. Development of Potent Glucagon-like
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104
Appendix Chapter 3: Supplementary Data
105
Figure A3.1 Inhibitor Selection Scheme a, Overview of the in vitro selection of a 13,824-
membered DNA-templated macrocycle library for IDE binding affinity18,19. b, Enrichment results
from two independent in vitro selections against N-His6-mIDE using the DNA-templated
macrocycle library18. The numbers highlight compounds enriched at least 2-fold in both
selections. c, Structures of IDE-binding macrocycles 1-6 decoded from DNA library barcodes
corresponding to building blocks A, B, C and D. The cis and trans isomers are labeled ‘a’ and
‘b’, respectively. The two isomers were synthesized as previously reported18,19 and separated
by HPLC. IDE inhibition activity was assayed by following cleavage of the fluorogenic peptide
substrate Mca-RPPGFSAFK(Dnp)-OH.
incubation with
immobilized target
PCR with Illumina
adaptor primers
high-throughput
DNA sequencing
millions of sequence reads
N-His6 mIDE
enriched library pool
1
2
3
4
5
6
1
23
4
5
6
IDE in vitro selection 1 results
IDE in vitro selection 2 results
a b
washing of non-
binding fraction
A2
B8
C6
A12
B8
D5 D5
C8
A12
B8
D6
C11
A12
B8
D5
C6
A2
B8
C11
D6
A12
B8
D5 C5
3a (cis olefin) IC50>20 µM
3b (trans olefin) IC50=1.5 µM
1 (cis olefin) IC50>100 µM
1 (trans olefin) IC50=5.0 µM
2a (cis olefin) IC50=10 µM
2b (trans olefin) IC50=0.14 µM
4a (cis olefin) IC50>100 µM
4b (trans olefin) IC50>100 µM
5a (cis olefin) IC50>20 µM
5b (trans olefin) IC50=1.0 µM
6a (cis olefin) IC50=5.6 µM
6b (trans olefin) IC50=0.06 µM
c IDE in vitro selection hits
IDE in vitro selection
106
Figure A3.2 Inhibition of human and mouse IDE activity demonstrated using distinct
assays. a and b, cleavage of the fluorogenic substrate peptide Mca-RPPGFSAFK(Dnp)-OH by
human and mouse IDE in the presence of inhibitors (a) 6b and (b) 6bK. c, Homogeneous time-
resolved fluorescence (HTRF, Cisbio) assay measuring degradation of insulin by IDE (R&D) in
the presence of 6b, 6bK and 28. d, LC-MS assay for ex vivo degradation of CGRP (10 µM) by
endogenous IDE in mouse plasma in the presence of 6b. e and f, Biochemical assays
suggesting that 6b binds a site in IDE distinct from the conventional peptide substrate binding
site known to bind substrate mimetic Ii1. Yonetani–Theorell double inhibitor plots of IDE activity
in the presence of (e) 6b and Ii1, or (f) 6b and bacitracin. Crossing lines indicate synergistic
and independent binding of inhibitors, while parallel lines indicate competition for binding to the
enzyme. The inhibitors assayed using the fluorogenic substrate Mca-RPPGFSAFK(Dnp)-OH.
0%
20%
40%
60%
80%
100%
0.001 0.01 0.1 1 10
insu
lin d
eg
rad
atio
n (
%)
inhibitor concentration (µM)
6b
28
6bK
0%
20%
40%
60%
80%
100%
DMSO 0.1 µM 0.3 µM 1 µM 3 µM 10 µM
plasma + inhibitor 6b
CGRP cleavage (ex vivo plasma, LCMS assay)Insulin degradation (in vitro, HTRF assay)c d
0%
20%
40%
60%
80%
100%
0.001 0.01 0.1 1 10
IDE
in
hib
itio
n (
%)
6b concentration (µM)
0%
20%
40%
60%
80%
100%
0.001 0.010 0.100 1.000 10.000
IDE
in
hib
itio
n (
%)
6bK concentration (µM)
human IDE
mouse IDE
human IDE
mouse IDE
a bFluorogenic peptide degradation (6b inhibition) Fluorogenic peptide degradation (6bK inhibition)
CG
RP
cle
ava
ge
(%
)6bK
28
6b
e
0.0
0.5
1.0
1.5
2.0
2.5
3.0
3.5
4.0
4.5
-0.20 0.00 0.20 0.40 0.60 0.800.0
0.5
1.0
1.5
2.0
2.5
0.00 0.02 0.04 0.06 0.08
5.0 nM (9x IC50)
1.7 nM (3x IC50)
0.6 nM (1x IC50)
0.2 nM (1/3x IC50)
Ii1 concentration:
6b concentration (μM)
1/v
(x1
0-4Δ
A/m
in)
(n = 4)
90 µM (9x IC50)
30 µM (3x IC50)
10 µM (1x IC50)3.3 µM (1/3x IC50)
6b concentration (μM)
1/v
(x1
0-4Δ
A/m
in)
(n = 4)
Bacitracin concentration:
f Double inhibitor plot for 6b and bacitracinDouble inhibitor plot for 6b and Ii1
107
Figure A3.3 Data collection and refinement statistics (molecular replacement), docking
simulation for 6b, and competition test between insulin and fluorescein-labeled
macrocycle 31 for binding CF-IDE. a, One crystal was used to solve the CF-IDE•6b structure.
The highest-resolution shell is shown in parentheses. Structure coordinates are deposited in
the Protein Data Bank (accession number 4TLE). b, Molecular docking simulations are
consistent with the placement of building blocks A and B in the structural model. The structure
108
of 6b in binding site from crystallographic data with composite omit map contoured at 1.0 σ (p-
benzoyl-phenylalanine is shown in red, cyclohexylalanine in blue, and the backbone in purple).
c, Highest-scoring pose from DOCK simulations (glutamine group is shown in green). d,
Residue decomposed energy of the crystal (green) and docked (blue) poses of 6b. e,
Competition test between the fluorescein-labeled macrocycle 31 and insulin for binding CF-IDE.
Cysteine-free catalytically-inactive IDE was titrated against 0.9 nM macrocycle 31 alone () or
together with 2.15 μM insulin (), producing a shift in apparent dissociation constant for
macrocycle 31 according to equation Eq. 1 (Supplementary Information). Representative
fluorescence polarization plots are shown.
109
Figure A3.4 Small molecule-enzyme mutant complementation study to confirm the
macrocycle binding site and placement of the benzophenone and cyclohexyl building-
block groups. a, IDE mutant A479L is inhibited by 6b >600-fold less potently compared to
wild-type IDE. b, Analog 9, in which the p-benzoyl ring is substituted for a smaller tert-butyl
group, inhibits A479L IDE and WT IDE comparably. c, Similarly, IDE mutant G362Q is inhibited
77-fold less potently by 6b compared with WT IDE. d, Analog 13, in which the L-cyclohexyl
alanine side chain was substituted with a smaller L-leucine side chain, inhibits G362Q IDE and
WT IDE comparably. The full list of IDE mutants investigated is shown in Supplementary Table
S5.
NH
O
HN O
HN
O
HN
O
NH
O
H2N
O
O
NH2O
G362Q
NH
O
HN O
HN
O
HN
O
NH
O
H2N
O
NH2O
A479L
9
13
a
0%
20%
40%
60%
80%
100%
0.001 0.01 0.1 1 10 100
IDE
inh
ibit
ion
(%
)
6b concentration (µM)
hIDE A479L
hIDE WT
0%
20%
40%
60%
80%
100%
0.001 0.01 0.1 1 10 100
IDE
inh
ibit
ion
(%
)
6b concentration (µM)
G362Q - 6b
WT2 - 6b
0%
20%
40%
60%
80%
100%
0.001 0.1 10 1000
IDE
inh
ibit
ion
(%
)
13 concentration (µM)
G362Q - 40
WT2 - 40
0%
20%
40%
60%
80%
100%
0.1 1 10 100 1000 10000
IDE
inh
ibit
ion
(%
)
9 concentration (µM)
hIDE A479L
hIDE WT
6b inhibits A479L mutant
poorly versus wild-type IDE
9 inhibits A479L and WT
IDE comparably
A479L
WT
A479L
WT
G362Q
WT
G362Q
WT
ß77xà
ß >600x à
b
6b inhibits G362Q mutant
poorly versus wild-type IDE
13 inhibits G362Q and WT
IDE comparably c d
110
Figure A3.5 Pharmacokinetic parameters of 6bK. a, Plasma binding, plasma stability, and
microsomal stability (1 h incubation) data was provided by Dr. Stephen Johnston and Dr. Carrie
Mosher (Broad Institute). b, Heavy 6bK was synthesized with 15N,13C-lysine for stable-isotope
dilution LC-MS quantitation. c Concentration of 6bK in mice tissues and plasma collected over
4 hours (n = 1-2). d, Average biodistribution of 6bK in five lean mice at 150 min post-injection
of 6bK 80 mg/kg i.p. at the endpoint of a IPGTT experiment. We did not detect 6bK in the brain
even using 10-fold concentrated samples for LC-MS injection compared to other tissues.
experimental window
0
50
100
150
200
250
300
brain panreas liver kidney blood
6b
K (µ
g/g
tis
su
e)
6bK levels 150 min. post-injection
0
50
100
150
200
250
300
0 30 60 90 120 150 180 210 240
6b
K (µ
g/g
tis
su
e)
time post-injection of 6bK (min)
Brain
Pancreas
Kidney
Liver
Blood
6bK biodistribution 4 h time-course post-injection
(n = 5)
0
100
200
300
400
500
6b
K c
on
c. (µ
M)
0
100
200
300
400
500
6b
K c
onc. (µ
M)
c d
SamplePlasma
binding
Plasma
stability (1 h)
Microsomal
stability (1 h)
mouse 94 % 74 % 78 %
human 86 % 83 % 80 %
a b
heavy 6bK
(stable isotope
dilution standard)
6bK stability ex vivo
111
Figure A3.6 Dose tolerance, augmented insulin hypoglycemic action by 6bK in mice, and
unaffected amyloid peptide levels in the mouse brain. a, Body weight measurements for
C57BL/6J mice treated with 6bK (, 80 mg/kg i.p.) or vehicle alone (). Mice treated with 6bK
(, 80 mg/kg) are active, display normal posture, normal grooming, and response to stimulation.
b, Increased hypoglycemic response to a high dose of insulin (1.0 U/kg) under acute IDE
inhibition (compare with Fig. 4b). Non-fasted male C57BL/6J mice were treated with a single
i.p. injection of IDE inhibitor 6bK (, 80 mg/kg) or vehicle alone (), followed by i.p. insulin
(Humulin-R, 1.0 U/kg). The animals in the 6bK-treated cohort experienced lethargy and
hypothermia consistent with the augmented effect of insulin. c and d, Treatment of C57BL/6J
lean mice with 6bK (, 80 mg/kg, n = 6) does not change brain levels of Aβ(40) or Aβ(42)
peptides in the brain 2 h post injection compared to treatment with vehicle alone (, n = 5) or
inactive diastereomer bisepi-6bK (, 80 mg/kg, n = 6). All data points and error bars represent
mean ± SEM.
0
50
100
150
200
-60 -30 0 30 60
6bK (80 mg/kg)
Vehicle
Rx insulin
blo
od
glu
co
se (
mg/d
L)
min. post-insulin injection (1 U/kg)
0
5
10
15
20
25
30
0 1 3
bodyw
eig
ht
(g)
days post GTT experiment
Vehicle (n = 7) 6bK (80 mg/kg) (n = 7)
(n = 8-9)
ba6bK injection is well tolerated 6bK augments insulin action in vivo
dcBrain Aβ(40) leves 2 h post-injection Brain Aβ(42) leves 2 h post-injection
0
0.1
0.2
0.3
0.4
Veh 6bK bisepi Veh 6bK bisepi Aβ
(42
) pm
ol/g b
rain
0
0.2
0.4
0.6
0.8
1.0
1.2
1.4
Aβ
(40)
pm
ol/g
bra
in
****
112
Figure A3.7 Dependence of insulin and glucagon secretion on the route of glucose
administration (oral or i.p.) due to the both the ‘incretin effect’ as well as the
hyperinsulinemic phenotype of DIO versus lean mice. a, The early insulin response to
glucose in lean and DIO mice is higher during OGTT than IPGTT. b, Suppression of glucagon
secretion post-glucose administration is less effective after IPGTT and in DIO mice. All data
points and error bars represent mean ± SEM. Statistics were performed using a two-tail
Student’s t-test, and significance levels shown in the figures are * p < 0.05 or ** p < 0.01
between the labeled groups.
0.0
2.0
4.0
6.0
8.0
0.00
0.03
0.06
0.09
0.12
pla
sm
a in
su
lin (
ng
/mL
)
oral
pla
sm
a g
lucag
on
(ng/m
L)
lean mice DIO mice
insulin response, 20 min post-glucose
i.p. oral i.p.
lean mice DIO mice
glucagon response, 135 min post-glucose
glucose administration routeglucose administration route
a b
oral i.p. oral i.p.
* **
**
113
Figure A3.8 Low-potency diastereomers of 6bK used to determine effective dose range of
2 mg/mouse and confirm on-target IDE inhibition effects during IPGTTs in lean and DIO
mice. a, Inhibition of mouse IDE activity by low potency diastereomers of 6bK. The
stereocenters altered in each compound relative to those of 6bK are labeled with a star. b, The
effects of 6bK (, 90 mg/kg) were compared to the weakly active stereoisomer epi-C-6bK (,
90 mg/kg) and vehicle controls () during an ipGTT to determine the dosing range in lean mice.
c, Two doses of 6bK, 80 mg/kg () and 40 mg/kg () were compared with inactive bisepi-6bK
(, 80 mg/kg) and vehicle alone (). d and e, Administration of 6bK (, 80 mg/kg) to lean mice
not followed by injection of a nutrient such as glucose or pyruvate did not significantly alter (d)
basal blood glucose or (e) basal hormone levels compared to bisepi-6bK () or vehicle controls
IC50 ~ 1.5 µM
epi-C-6bK
IC50 = 100 µM IC50 > 200 µM
bisepi-6bK
***
*
epi-B-6bK
0%
20%
40%
60%
80%
100%
0.001 0.01 0.1 1 10 100 1000
mo
use ID
E inhib
itio
ninhibitor concentration (µM)
6bK
epi-C
epi-B
bis-epi
6bK
epi-C-6bK
epi-B-6bK
bisepi-6bK
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
epi-C (90 mg/kg)
6bK (90 mg/kg)
Vehicle
**
*
*
Rx
i.p.
glucose
**
**
**
(n = 4-5)
blo
od g
luco
se
(m
g/d
L)
b
6bK
epi-C
c
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
6bK (80 mg/kg)
6bK (40 mg/kg)
bisepi (80 mg/kg)
Vehicle
**
*
*
Rxi.p.
glucose
(n = 5-6)
6bK
bisepi
6bK
a
d e
0
100
200
300
-60 -30 0 30
blo
od g
luco
se
(m
g/d
L)
minutes (relative to GTTs)
bisepi (80 mg/kg)
6bK (80 mg/kg)
Vehicle
Rx
(n = 7)
0.00
0.05
0.10
0.15
0.20
0.0
0.5
1.0
1.5
2.0
0.00
0.05
0.10
0.15
0.00
0.25
0.50
0.75
1.00ho
rmone (
pg/m
L)
Glucagon
Insulin
Amylin
C-peptideho
rmo
ne (
pg/m
L)
V 6bK bis
epi
V 6bK bis
epi
unchanged blood glucose
after 6bK injection alone
unchanged hormones levels
after 6bK injection alone
6bK
bisepi
lean mice, IPGTT lean mice, IPGTT
low potency 6bK diastereomer controls
114
(). All data points and error bars represent mean ± SEM. Statistics were performed using a
two-tail Student’s t-test, and significance levels shown in the figures are * p < 0.05 versus
vehicle control group; ** p < 0.01 versus vehicle control group.
115
Figure A3.9 Relative area under the curve calculations and 6bK dose response for the
glucose tolerance tests shown in Fig. 3.3. a, During OGTT, lean and DIO mice treated with
6bK (, 2 mg/animal) display improved glucose tolerance (lower blood glucose area), compared
to vehicle controls () and inactive bisepi-6bK (). b, In contrast, during IPGTT both lean and
DIO mice treated with 6bK () display impaired glucose tolerance (higher blood glucose area)
compared to vehicle () or bisepi-6bK () controls. c and d, Dose-response of 6bK (40 and
90 mg/kg; see Fig. 3d for 60 mg/kg) followed by IPGTT in DIO mice. Vehicle alone () and a
matching dose of bisepi-6bK () were used as controls. c, DIO mice treated with low doses of
6bK (, 40 mg/kg) responded to IPGTT in either of two ways: improved glucose tolerance
throughout the experiment (n = 3) or a hyperglycemic rebound as described in the main text (n =
0%
50%
100%
150%
200%
0%
25%
50%
75%
100%
125%
0%
25%
50%
75%
100%
125%
OGTT blood glucose profile areas
0%
50%
100%
150%
200%
lean mice DIO mice
IPGTT blood glucose profile areas
lean mice DIO mice
a b
rela
tive b
lood
glu
cose
are
a
rela
tive b
lood g
luco
se a
rea
V 6bK bis
epi
V 6bK bis
epi
V 6bK bis
epi
V 6bK bis
epi
*
*
**
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
bisepi (90 mg/kg)
6bK (90 mg/kg)
Vehicle
**
Rx
i.p.
glucose
(n = 5)
*
****
0
100
200
300
400
-60 -30 0 30 60 90 120
minutes post-glucose injection (1.5 g/kg)
bisepi (40 mg/kg)
6bK (40 mg/kg)
Vehicle
*
Rx
i.p.
glucose
**
(n = 7)
blo
od
glu
co
se (
mg/d
L)
‘rebound’, n = 4
no ‘rebound’, n = 3
c d
blo
od
glu
co
se
(m
g/d
L)
IPGTT, DIO mice, low 6bK dose IPGTT, DIO mice, highest 6bK dose
116
4), suggesting this dose is too low to achieve a consistent effect (note the large error bars). d,
Mice treated with high doses of 6bK (, 90 mg/kg) respond similarly to 60 mg/kg (Fig. 3d), but
the potential weak activity observed for bisepi-6bK (IC50 > 100 µM) at this high dose ()
compared to vehicle alone () suggests that 90 mg/kg may be too high. All data points and
error bars represent mean ± SEM. Statistics were performed using a two-tail Student’s t-test,
and significance levels shown in the figures is * p < 0.05 versus vehicle control group. See the
Supplementary Methods section for a description of the AUC calculation.
117
Figure A3.10 Oral glucose tolerance of mice lacking IDE compared to WT lean mice, and
lack of effect of 6bK treatment in IDE–/– knockout mice. a, Mice lacking IDE treated with 6bK
(, 80 mg/kg, i.p.) followed by oral glucose produce an identical response compared to vehicle-
treated controls () of the same genotype (IDE–/–). b, Transient IDE inhibition in age-matched
IDE+/+ WT control mice treated with 6bK (, 80 mg/kg, i.p.) display improved oral glucose
tolerance compared to vehicle-treated controls () of the same genotype (similar to Fig. 3a). c,
In contrast, when mice lacking IDE (, IDE–/–) are compared with age-matched IDE+/+ controls
() the IDE knockout mice display impaired oral glucose tolerance, supporting the hypothesis
that chronic deletion of IDE leads to pronounced compensatory changes in metabolism that are
not predictive of the outcome of IDE inhibition.10,11 All data points and error bars represent
mean ± SEM. Statistics were performed using a two-tail Student’s t-test, and significance level
shown in the figures is * p < 0.05 versus WT vehicle control group.
oral glucose, IDE+/+ mice oral glucose, IDE–/– mice
0
100
200
300
400
-60 -30 0 30 60 90 120
IDE -/-, 6bK (80 mg/kg)
IDE -/-, Vehicle
Rx
oral
glucose
(n = 5-7)
0
100
200
300
400
-60 -30 0 30 60 90 120
IDE +/+, 6bK (80 mg/kg)
IDE +/+, Vehicle
Rx
oral
glucose
*
(n = 8-9)
minutes post-glucose gavage (3.0 g/kg)
blo
od g
luco
se
(m
g/d
L)
minutes post-glucose gavage (3.0 g/kg)
0
100
200
300
400
-60 -30 0 30 60 90 120
IDE -/-, Vehicle
IDE +/+, Vehicle
Rx
oral
glucose
*
*
(n = 5-9)
minutes post-glucose gavage (3.0 g/kg)
oral glucose, IDE–/– vs IDE+/+ mice a b c
118
Supplementary Figure S1. Western blot for IDE using whole blood lysate (0.5 µL/well) from
IDE–/– mice and a wild-type (WT) control sample.
L WT
33
0.6
33
4.4
33
4.5
33
4.6
33
5.2
33
5.3
33
5.4
33
6.2
33
6.3
L WT
341
.3
341
.4
345
.5
347
.4
347
.5
347
.6
350
.3
350
.4
352
.3
150
100
75
50
37
150
100
75
50
37
IDE-/- KO mice IDE-/- KO mice
119
Supplementary Scheme S1. Fmoc-based solid-supported synthesis of 6bK followed by on-
resin macrocyclization.
120
IDE substrates in vitro (reference)
Alternative degrading enzymes (Brenda db)
kcat
(min-1)
KM (µM)
kcat/
KM IC50 (µM)
X-ray struct.
IDE substrate in vivo (ref.)
insulin 28,29
lysosomal proteases, disulfide reductase
1.52 <0.03 50 - 2WBY
KO study 30,31
2WC0
Aβ (40, 42) 32,33
NEP, cathepsin D 52 1.23 43 - 2G47
KO study 30,34,35
2WK3
calcitonin-gene related peptide
6
ECE, PREP - - - - - KO study 6
glucagon 36,37
NEP, nardilysin, DPP-IV, cathepsins B and C
38.5 3.46 11 weak 2G49 this study
amylin 38
- n/a 0.3* n/a 0.16 3HGZ
this study 2G48
TGF-α 39
- - 0.15* - 0.08 3E50 -
IGF-1 34,40
DPP-IV - weak - - - -
IGF-2 34,40
- - 0.1* - 0.06 3E4Z -
somatostatin-14 41
nardilysin, dactylysin, aminopeptidase B, THOP, neurotensin-degrading enzyme
22.8 7.5 3.0 - - -
bradykinin 42
ACE, aminopeptidase P, carboxypeptidase N, NEP, DPP-II, DPP-IV,
- 4.2 - - 3CWW -
kallidin 42
ACE, aminopeptidase P, carboxypeptidase N
- 7.3 - - - -
atrial NP (ANP) 43,44
NEP - 0.06 - - 3N57 -
B-type NP (BNP) 44
NEP, fibroblast activation protein-α
- weak - >1 3N56 -
relaxin 45
- - 0.11* - 0.054 - -
relaxin-3 45
- - 0.36* - 0.182 - -
insulin-like peptide 3 46
- 0.15 0.055 2.7 - - -
β-endorphin (1-31) 42
NEP 21 13 1.6 - - -
growth hormone releasing factor (1−29)
42
DPP-IV, NEP 23.4 11.9 2.0 - - -
pancreastatin (1-49) 42
- 10.6 41.7 0.25 - - -
dynorphin B (1-13) 42
NEP 15.1 18.3 0.8 - - -
A (1-17) 42
NEP 18.4 37.4 0.5 - - -
B (1-9) 42
NEP 10.3 26.8 0.4 - - -
A (1-13) 42
NEP 3.74 40.6 0.09 - - -
A (1-10) 42
NEP 3.74 39.4 0.09 - - -
A (1-8) 42
NEP 0.66 63.5 0.01 - - -
A (1-9) 42
NEP 0.33 60.5 0.01 - - -
Table A3.1 Literature survey of putative IDE substrates identified using in vitro assays.
(*) KM estimated based on IC50 for inhibition of insulin degradation. Abbreviations: Aβ = amyloid
beta; TGF-alpha = transforming growth factor-alpha; IGF = insulin-like growth factor; NP =
natriuretic peptide; GRF = gastrin release factor; NEP = neprilysin; PREP = prolyl
endopeptidase; ECE = endothelin converting enzyme; THOP = thimet oligopeptidase; ACE =
angiotensin-converting enzyme; DPP = dipeptidylpeptidase. Known non-substrates of IDE
include glucagon-like peptide 1 (GLP-1), glucose-dependent insulinotropic peptide (GIP),
epithelial growth factor 1 (EGF-1) and C-peptide.
121
Compound Purity (%) Formula [M+H]+ expected
[M+H]+ found
Ion count Δ (ppm)
1a 87.5 C26H41N7O7 564.3140 564.3135 17505 -0.886 1b 66.4 C26H41N7O7 564.3140 564.3141 237080 0.177 2a 84.1 C41H55N9O7 786.4297 786.4290 523007 -0.890 2b 95.3 C41H55N9O7 786.4297 786.4272 627894 -3.179 3a 84.3 C46H62N6O8 827.4702 827.4703 111258 0.121 3b 89.9 C46H62N6O8 827.4702 827.4703 26066 0.121 4a 93.7 C32H52N6O7 633.3970 633.3975 1344574 0.789 4b 79.7 C32H52N6O7 633.3970 633.3967 591800 -0.474 5a 97.1 C41H52N6O7 741.3970 741.3987 517852 2.293 5b 75.4 C41H52N6O7 741.3970 741.3967 208124 -0.405 6a 98.3 C40H51N7O8 758.3872 758.3886 875721 1.846 6b 98.9 C40H51N7O8 758.3872 758.3878 14154 0.791 7 89.6 C40H53N7O7 744.4079 744.4079 21411 -0.040 8 94.9 C33H47N7O7 654.3610 654.3606 413032 -0.611 9 80.1 C37H55N7O7 710.4236 710.4239 180420 0.422 10 76.9 C39H51N7O7 730.3923 730.3917 644559 -0.821 11 92.6 C40H45N7O8 752.3402 752.3399 77585 -0.399 12 96.0 C37H47N7O8 718.3559 718.3550 145796 -1.253 13 95.7 C37H47N7O9 718.3559 718.3569 24610 1.392 14 58.2 C34H41N7O8 676.3089 676.3082 400965 -1.035 15 77.5 C38H48N6O7 701.3657 701.3671 124002 1.996 16 67.3 C38H48N6O7 701.3657 701.3683 19335 3.707 17 83.2 C39H50N6O7 715.3814 715.3808 298036 -0.839 18 92.3 C39H50N6O7 715.3814 715.3832 701250 2.516 19 37.4 C38H48N6O8 717.3606 717.3586 128261 -2.788 20 74.5 C37H46N6O7 687.3501 687.3503 135532 0.291 21 95.6 C40H50N6O9 759.3712 759.3726 13461 1.844 22 97.9 C40H52N6O8S 777.3640 777.3634 121542 -0.772 23 88.5 C40H52N6O7Se 807.3144 807.3139 1497 -0.619 24 52.4 C44H52N6O7 777.3970 777.3981 15952 1.415 25 63.5 C35H43N5O6 630.3286 630.3282 136628 -0.635 26 74.4 C40H51N7O8 758.3872 758.3876 119065 0.527 27 90.9 C39H49N7O8 744.3715 744.3708 210827 -0.940 29 75.3 C42H55N7O8 786.4185 786.4178 234651 -0.890 28 94.3 C40H50N6O9 759.3712 759.3705 89863 -0.922 30 97.5 C54H75N9O11S 1058.5380 1058.5402 23247 2.078 31 81.6 C65H71N7O15 1190.5081 1190.5063 442 -1.512 6bK 96.6 C41H55N7O7 758.4236 758.4233 501430 -0.396 heavy-6bK 96.4 C35
13C6H55N5
15N2O7 766.4378 766.4388 227096 1.305
bisepi-6bK 96.7 C41H55N7O7 758.4236 758.4232 133009 -0.527 epiA-6bK 96.6 C41H55N7O7 758.4236 758.4258 1320288 2.901 epiB-6bK 94.9 C41H55N7O7 758.4236 758.4235 216951 -0.132 epiC-6bK 93.9 C41H55N7O7 758.4236 758.4235 177995 -0.132 Ii1 94.8 C37H45N9O8 744.3464 744.3474 662 1.343
Table A3.2 HPLC and high-resolution mass spectrometry analysis of IDE inhibitor analogs.
122
Mutation Primers (forward, reverse)
A198Q ACATGAGAAGAATGTGATGAATGA-dU-CAGTGGAGAC
ATCATTCATCACATTCTTCTCATG-dU-TCTG
A198T AGACTCTTTCAATTGGAAAAAGC-dU-ACAGGG
AGCTTTTTCCAATTGAAAGAGTC-dU-CCAGGTATCATTCATCACATTCTTCTCATGTTC
A198C AGACTCTTTCAATTGGAAAAAGC-dU-ACAGGG
AGCTTTTTCCAATTGAAAGAGTC-dU-CCAGCAATCATTCATCACATTCTTCTCATGTTC
A198Y ACATGAGAAGAATGTGATGAATGA-dU-TACTGGAGAC
ATCATTCATCACATTCTTCTCATG-dU-TCTG
W199L ACATGAGAAGAATGTGATGAATGA-dU-GCCTTAAGACTC
ATCATTCATCACATTCTTCTCATG-dU-TCTG
W199F AGACTCTTTCAATTGGAAAAAGC-dU-ACAGGG
AGCTTTTTCCAATTGAAAGAGTC-dU-GAAGGCATCATTCATCACATTCTTCTC
W199Y AGACTCTTTCAATTGGAAAAAGC-dU-ACAGGG
AGCTTTTTCCAATTGAAAGAGTC-dU-ATAGGCATCATTCATCACATTCTTCTC
F202L ACATGAGAAGAATGTGATGAATGA-dU-GCCTGGAGACTCTTGCAATTG
ATCATTCATCACATTCTTCTCATG-dU-TCTG
F202R AGACTCTTTCAATTGGAAAAAGC-dU-ACAGGG
ATGAATGATGCCTGGAGAC-dU-CCGTCAATTGGAAAAAGCTACAGGG
I310R ACCCATTAAAGATCGTAGGAATC-dU-CTATGTGACATTTCCCATAC
AGATTCCTACGATCTTTAATGGG-dU-ACTATTTTGTAAAGTTGTTTAAG
Y314F ACCCATTAAAGATATTAGGAATCTC-dU-TCGTGACATTTCCCATACCTGACCTTC
AGAGATTCCTAATATCTTTAATGGG-dU-ACTATTTTG
V360Q AAAGGGCTGGGTTAATACTCT-dU-CAGGGTGGGCAG
AAGAGTATTAACCCAGCCCTT-dU-GACTTAAG
V360R AAAGGGCTGGGTTAATACTCT-dU-AGGGGTGGGCAGAAGGAAGGAGC
AAGAGTATTAACCCAGCCCTT-dU-GACTTAAG
G361Q AAAGGGCTGGGTTAATACTCT-dU-GTTCAGGGGCAGAAGGAAGGAGCCC
AAGAGTATTAACCCAGCCCTT-dU-GACTTAAG
G362Q AAAGGGCTGGGTTAATACTCT-dU-GTTGGTCAGCAGAAGGAAGGAGCCCGAG
AAGAGTATTAACCCAGCCCTT-dU-GACTTAAG
K364A AAGGAGCCCGAGGTTTTA-dU-GTTTTTTATC
ATAAAACCTCGGGCTCCT-dU-CCGCCTGCCCACCAACAAGAGTATT
I374M ATGTTTTTTATCATGAATGTGGACT-dU-GACCG
AAGTCCACATTCATGATAAAAAACA-dU-AAAACCTC
I374Q ATGTTTTTTATCCAGAATGTGGACT-dU-GACCGAGGAAGG
AAGTCCACATTCTGGATAAAAAACA-dU-AAAACCTCGGGCTCC
A479L ATGTCCGGGTTCTGATAGTTTCTAAA-dU-CTTTTGAAGGAAAAACTG
ATTTAGAAACTATCAGAACCCGGACA-dU-TTTCTGGTCTGAG
Table A3.3 Site-directed mutagenesis primers.
123
Sequencing primers
Seq_Fw1 GATTAACTTTATTATTAAAAATTAAAGAGG
Seq_Re1 CAACATGTAATAATCCTTCCTCGGTC
Seq_Fw2 GCATGAAGGTCCTGGAAGTCTG
Seq_Re2 AGGAAGGGTTACATCATCCAGAGC
Seq_Fw3 CCATGTACTACCTCCGCTTGC
Seq_Re3 GCAGATCTCGAGCTCGGATC
Seq_Fw4 GCTTATGTGGACCCCTTGCACTG
RT-PCR primers26,27
PEPCK_1_Fw GAACTGACAGACTCGCCCTATGT
PEPCK_1_Re GTTGCAGGCCCAGTTGTTG
G6Pase_1_Fw GTGCAGCTGAACGTCTGTCTGT
G6Pase_1_Re TCCGGAGGCTGGCATTGT
PEPCK_2_Fw GGTGTTTACTGGGAAGGCATC
PEPCK_2_Re CAATAATGGGGCACTGGCTG
G6Pase_2_Fw CATGGGCGCAGCAGGTGTATACT
G6Pase_2_Re CAAGGTAGATCCGGGACAGACAG
Tubulin_Fw CCTGCTCATCAGCAAGATCC
Tubulin_Re TCTCATCCGTGTTCTCAACC
Beta-actin_ Fw CATCCGTAAAGACCTCTATGCCAAC
Beta-actin_Re ATGGAGCCACCGATCCACA
Table A3.4 Sequencing and RT-PCR primers.
124
Protein Batch Relative activity
Ii1 IC50 shift *
6b IC50 shift
13 IC50 shift
9 IC50 shift
Prediction
hIDE WT 1 1.0 1.0 1.0 1.0 1.0
hIDE WT 2 1.0 1.0 1.0 1.0 -
hIDE WT 3 1.0 1.0 1.0 1.0 -
A198Q 1 1.4 1.0 2.3 - -
A198T 2 1.5 1.0 16 13.6 - scaffold interaction
A198Y 2 2.3 1.1 0.5 - -
W199F 2 1.3 1.8 3.0 3.2 - modest interaction
W199Y 2 0.3 1.4 1.8 - -
F202L 1 0.7 1.7 1.7 2.3 -
F202R 2 0.9 1.1 3.7 4.1 - modest interaction
I310R 2 3.0 1.9 0.8 0.7 -
Y314F 2 3.5 1.0 1.2 - -
V360Q 1 2.6 0.9 1.5 - -
V360R 3 0.4 0.9 1.4 - -
G361Q 3 0.7 0.9 0.8 - -
G362Q 3 1.2 0.6 77 1.8 - cyclohexyl ring interaction
K364A 2 4.3 1.0 26 10.0 - scaffold interaction
I374M 1 4.3 1.0 0.7 - -
A479L 1 0.5 0.9 >600 - 1.0 p-benzoyl interaction
Table A3.5 Site-directed IDE mutants used in the small molecule-enzyme mutant complementation studies. * NB: Ii1 is not known to interact with any of these residues. Significant changes in IC50 for Ii1 were presumed to indicate misfolding or other non-inhibitor-specific protein structure changes. For example, W199L displayed an IC50 shift of 21-fold for Ii1, 13-fold for 6b, and 17-fold for analog 13.
125
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